Methods of reducing transplant rejection and cardiac allograft vasculopathy by implanting autologous stem cells

ABSTRACT

The invention provides novel methods of reducing transplant rejection and cardiac allograft vasculopathy in humans by employing the implantation of autologous progenitor cells into the transplanted donor heart. The autologous progenitor cells can be vascular progenitor cells (VPCs) and/or myocyte progenitor cells (MPCs) isolated from the recipient&#39;s explanted heart. Alternatively, bone marrow progenitor cells (BMPCs) isolated from the recipient may also be used.

CROSS REFERENCE TO RELATED APPLICATIONS

This application is a divisional of U.S. application Ser. No. 12/325,373, filed Dec. 1, 2008, now U.S. Pat. No. 8,124,071, which claims the benefit of U.S. Provisional Application No. 60/991,499, filed Nov. 30, 2007, both of which are herein incorporated by reference in their entireties.

FIELD OF THE INVENTION

The present invention relates generally to the field of cardiology, and more particularly relates to methods of reducing transplant rejection by implanting cardiac stem cells or bone marrow progenitor cells isolated from the recipient into the donor heart.

BACKGROUND OF THE INVENTION

The interaction between donor and recipient cells after transplantation has received great attention in an attempt to identify the basis of rejection and graft-versus-host disease (1-5). Cell migration from the allograft to the recipient results in systemic chimerism (6-8), and cell migration from the host to the transplanted organ results in chimerism of the organ (9, 10). Chimerism can be detected easily after sex-mismatched organ transplantation with FISH for the Y-chromosome (11-13) and several studies on cardiac chimerism have provided consistent results concerning the migration of progenitor cells (PCs) from the host to the graft (14-26). The sex-mismatched transplants make it possible to document and evaluate quantitatively a process that is part of cardiac homeostasis but it is otherwise not measurable in humans (27). After homing, host PCs undergo replication and differentiation, generating mature myocytes and vascular structures in the transplanted heart (14). Although there is little disagreement among authors in terms of the occurrence of this phenomenon, the magnitude of cardiac chimerism varies significantly in different reports (14-27). This discrepancy involves mostly ventricular myocytes and to a much lesser extent coronary vessels. For myocytes, the published values range from as high as 18% (14) to as low as 0.02% (15). Conversely, levels of endothelial cell chimerism and vessel formation have been shown to involve up to 22% of the coronary circulation (14, 25). In spite of these differences which previously have been discussed (27-31), the regenerated cardiomyocytes and coronary arterioles together with capillary profiles have normal morphology and are distributed predominantly in areas of intact donor myocardium (14). These data provide evidence that adult PCs contribute to the formation of solid-organ tissue cells (32-36), but leave unanswered the question whether the migrating cells arise from precursors in the atrial remnants of the recipient's heart or translocate from the recipient's bone marrow through the circulation to the transplanted organ (37).

After the first year, chronic loss of graft function (71) is the predominant cause of mortality in cardiac transplant patients (72). Inflammation and immune-mediated reactions (73) are responsible for the reduced sensitivity of myocytes to catecholamines, alterations in surface receptors, defects in ion-channels and depressed contractility (74, 75). Graft dysfunction is characterized by changes in the coronary arteries by a process termed cardiac allograft vasculopathy (CAV) (76). Although a causal relationship between reduced graft function and CAV remains to be demonstrated, the progressive occlusion of coronary vessels and ischemic myocardial damage are the critical mechanisms of graft failure (77-81). Several risk factors for CAV have been identified; they include systemic hypertension, body mass index, advanced donor age and number of rejection episodes (82-90). CAV inexorably leads to a chronic ischemic myopathy and death (91); 75% of transplant patients suffer from CAV one year following surgery (92, 93). Histologically, four etiologic factors have been considered: (a) intimal thickening mediated by migration of smooth muscle cells and/or proliferation of resident or migratory smooth muscle cells (94, 95); (b) infiltration of the intima by leukocytes recruited in response to injury or inflammation (96, 97); (c) accumulation of T lymphocytes and macrophages which generate a peri-vascular cuffing, local injury and irreversible damage, commonly defined as constrictive vascular remodeling (98-103); and (d) dynamic reduction in vessel diameter sustained by abnormalities in vasoconstriction and dilation (104-107). CAV differs from typical atherosclerotic lesions (108). With CAV, lesions are concentric and diffuse rather than eccentric and focal and extend beyond the large arteries reaching the penetrating smaller ramifications. Because of its diffuse distribution, CAV cannot be corrected with bypass surgery, angioplasty or stenting (72). In some cases, both types of lesions are present.

The cause of graft coronary artery disease remains elusive although immune and non-immune mechanisms have been implicated (70, 109). Controversy exists as to the origin of the proliferating cells present in CAV (110). It has been proposed that thickening of the intima is dictated by accumulation of recipient cells which derive from a pool of circulating PCs that differentiate locally into endothelial cells (ECs) and smooth muscle cells (SMCs) (111). Endothelial progenitor cells (EPCs) from the recipient may home to the intima and differentiate into endothelial-like cells (112-118) contributing to the vascular lesion. Similarly, SMC precursors could be recruited from the circulation and participate in vessel pathology (119-124). The results of cardiac chimerism in humans, however, question the negative effects of PCs of recipient origin (14, 15, 19, 20, 23, 25). There is general agreement that these cells contribute minimally to CAV and the formed coronary vasculature is structurally intact with no signs of atherosclerosis. The opposite view is supported by animal studies in which the orthotopic aorta allograft has been employed (117, 125, 126). This model has limitations; the aorta is structurally different from the coronary arteries and its intramural branches (127-130). Most importantly, medial necrosis is present in the orthotopic aorta allograft (125, 126, 131-133) while it is never observed in human CAV. These differences raise questions on the appropriateness of this model for graft vascular disease. At present, a few effective pharmacological therapies have been applied to the treatment of CAV. The HMG-CoA reductase inhibitors and the cell cycle inhibitor rapamycin reduce neointimal proliferation, myocardial infarction, the need for revascularization and death (134, 135). These therapies are extremely valuable but only delay the progression of CAV in the transplanted heart. Cell therapy with the formation of coronary vessels (47, 48, 51-53, 56, 57, 59, 64, 65) may increase coronary blood flow (CBF), decrease coronary resistance and enhance tissue oxygenation (136). The problem in need of resolution involves the identification and characterization of PCs that can form large conductive coronary arteries and their distal branches together with a large quantity of cardiomyocytes (59, 64, 137).

SUMMARY OF THE INVENTION

The present invention provides a novel approach to reduce transplant rejection and cardiac allograft vasculopathy in humans. The inventors have discovered distinct classes of progenitor cells that create immunocompatible myocardium within the non-immunocompatible transplanted heart and improve myocardial performance, reduce morbidity-mortality and ultimately prolong life.

In some embodiments, the methods of the instant invention comprise delivery of cardiac progenitor cells isolated from the recipient into the transplanted donor heart, wherein the progenitor cells engraft and differentiate into myocytes, smooth muscle cells, and endothelial cells resulting in the formation of functionally-competent, immunocompatible myocardium and coronary vessels. Thus, the present invention provides a method of reducing an immune response to a transplanted donor heart in a subject. In one embodiment, the method comprises obtaining myocardial tissue from the subject's explanted heart; extracting cardiac progenitor cells from said myocardial tissue; expanding said cardiac progenitor cells in culture; and administering said cardiac progenitor cells to the transplanted donor heart, wherein said cardiac progenitor cells generate immunocompatible myocardium and immunocompatible myocardial vessels following their administration, thereby reducing the immune response to said transplanted donor heart. In another embodiment, the cardiac progenitor cells are separated into vascular progenitor cells and myocyte progenitor cells prior to administration. Vascular progenitor cells may be c-kit positive and flk1 positive, and differentiate into immunocompatible smooth muscle cells and endothelial cells. Myocyte progenitor cells may be c-kit positive and flk1 negative and differentiate into immunocompatible cardiomyocytes. In another embodiment, the method further comprises activating the cardiac progenitor cells prior to administration by exposing the cells to one or more cytokines.

In another embodiment of the invention, the method of reducing an immune response to a transplanted donor heart in a subject comprises obtaining a bone marrow specimen from the subject; extracting adult bone marrow progenitor cells from said specimen; expanding said bone marrow progenitor cells in culture; and administering said bone marrow progenitor cells to the transplanted donor heart, wherein said bone marrow progenitor cells generate immunocompatible myocardium and immunocompatible myocardial vessels following their administration, thereby reducing the immune response to said transplanted donor heart. In some embodiments, the bone marrow progenitor cells are c-kit positive. In another embodiment, the bone marrow progenitor cells are administered immediately after transplantation. In another embodiment, the bone marrow progenitor cells differentiate into immunocompatible endothelial cells, smooth muscle cells, and cardiomyocytes.

In another embodiment of the invention, the method further comprises extracting cardiac progenitor cells from said subject's explanted heart; separating said cardiac progenitor cells into vascular progenitor cells and myocyte progenitor cells; and administering said vascular progenitor cells and myocyte progenitor cells to the transplanted donor heart. The vascular progenitor cells and myocyte progenitor cells may be administered by multiple administrations after transplantation. The multiple administrations may occur at a set interval after administration of the bone marrow progenitor cells.

In another embodiment of the invention, the method of reducing an immune response to a transplanted donor heart in a subject comprises obtaining myocardial tissue from the subject's explanted heart; extracting cardiac myocyte progenitor cells from said myocardial tissue; expanding said myocyte progenitor cells in culture; and administering said myocyte progenitor cells to the transplanted donor heart, wherein said myocyte progenitor cells generate immunocompatible myocardium following their administration, thereby reducing the immune response to said transplanted donor heart. The myocyte progenitor cells may be c-kit positive and flk1 negative. In one embodiment, the myocyte progenitor cells differentiate into immunocompatible cardiomyocytes.

The present invention also provides a method of reducing cardiac allograft vasculopathy in a subject who has received a transplanted donor heart. In one embodiment, the method comprises obtaining myocardial tissue from the subject's explanted heart; extracting cardiac vascular progenitor cells from said myocardial tissue; expanding said vascular progenitor cells in culture; and administering said vascular progenitor cells to the transplanted donor heart, wherein said vascular progenitor cells generate immunocompatible coronary vasculature, thereby repairing/and or regenerating the non-immunocompatible coronary arteries of the donor heart. The vascular progenitor cells may be c-kit positive and flk1 positive. In one embodiment, the vascular progenitor cells differentiate into immunocompatible endothelial cells and smooth muscle cells.

In some embodiments, the methods described herein may further comprise administering to the subject an immunosuppressive therapy. The immunosuppressive therapy may be administered concurrently or subsequently to the administration of the progenitor cells to the donor heart. Preferably, the dose and frequency of a standard immunosuppressive therapy is reduced following the administration of one or more types of progenitor cells (e.g. bone marrow progenitor cells, vascular progenitor cells, or myocyte progenitor cells) to the donor heart.

BRIEF DESCRIPTION OF THE DRAWINGS

FIG. 1. Administration of progenitor cells (PCs) to the cardiac transplant. Bone marrow is harvested from the recipient male dog and mononuclear cells are lineage depleted and sorted for c-kit (BMPCs). Following transplantation of a female donor heart, the explanted heart from the recipient is dissociated and vascular progenitor cells (VPCs) and myocyte progenitor cells (MPCs) are isolated and expanded. PC classes will be infected with a lentivirus expressing EGFP, β-gal or RFP for the subsequent identification of the injected cells and their progeny at different time points. Newly formed EGFP-, β-gal and RFP-positive myocardial structures will develop within the donor myocardium. Since labeled-PCs are given repeatedly over time, the coronary route is considered the most feasible form of cell delivery.

FIG. 2. Cardiac chimerism. A 67-year-old man died 9 days after sex mismatched heart transplant. The donor female heart showed regeneration foci characterized by clusters of developing myocytes. A-D: α-SA: red; nuclei: DAPI, blue. Myocyte boundaries were defined by laminin (yellow). The analysis of sex-chromosomes by FISH documented the male genotype of the new myocytes (arrows) which carried at most one Y-chr (green-dots) and one X-chr (magenta-dots). Large myocytes (asterisks) had a female genotype (two X-chr). A: one new myocyte contained two sets of X- and Y-chr suggesting cell fusion (double arrows). However, phospho-H3 (inset, white) demonstrated mitotic division and excluded cell fusion. Similar examples were found in other transplanted hearts.

FIG. 3. Chimerism of the dog heart. Donor female heart transplanted in male recipient. Subsequently the donor heart was injected with autologous-recipient EGFP-positive PCs. Several small developing myocytes are present (A, B: α-SA: red). These new myocytes are also EGFP-positive (B: α-SA-EGFP, yellow). Three of these cells are shown at higher magnification in the inset (B). Analysis of sex-chromosomes documented the male genotype of the forming myocytes (arrows) which carried at most one Y-chr (white dots) and one X-chr (magenta dots). Female recipient myocytes show at most two X-chr (*).

FIG. 4. Transplanted dog heart. A, B: Areas of myocardial damage occupied by inflammatory cells. C: These cells are CD4 (B lymphocytes) and CD8 (T lymphocytes) positive. D-F: Lymphocytic infiltrates in the luminal and abluminal aspects of a large and intermediate branch of LAD.

FIG. 5. Dog heart: vascular and myocardial niches. A: Resistance coronary arteriole; c-kit-positive cells (green) are present in the intima (vWf, yellow, *), SMC layer (α-SMA, red, arrows) and adventitia (not stained, arrowheads). B: The c-kit-positive-cells express flk1 (white), i.e., VPC niche. C, D: Tangential section of myocardial capillaries that exhibit 3 c-kit-positive flk1-positive VPCs. Connexin 43 (yellow, arrows) is present between VPCs and ECs. E: Large section of a dog coronary artery (SMCs, α-SMA; red). Area in the rectangle is shown in panel F: 2 VPCs are connected to SMCs. The inset illustrates connexin 43 (yellow, arrows). (G, H: LV myocardium which shows a cluster of c-kit-positive flk1-negative cells (green), i.e., MPC niche. Connexin 43 (arrowheads) and N-cadherin (arrows) are present between two MPCs, and between MPCs and myocytes (α-SA, red) or MPCs and fibroblasts (procollagen, light blue).

FIG. 6. PC classes. Freshly isolated dog BMPCs, and VPCs and MPCs expanded in vitro (P3-P4). A: BMPCs were stained with antibodies for blood lineages. B: Lineage negative c-kit-positive BMPCs were identified and sorted and analyzed in cytospin preparations; c-kit (green). C: VPCs are positive for c-kit and flk1 and negative for hematopoietic markers and α-SA; they express at very low levels desmin, CD31, vWf and TGF-β1 receptor. D: VPCs are c-kit-positive (green) and flk1-positive (red). E: MPCs are negative for flk1 and for hematopoietic markers, CD31, vWf and TGF-β1 receptor; they express at very low levels α-SA and desmin. F: MPCs are c-kit-positive (green) and flk1-negative.

FIG. 7. Clones and derived progeny. Single VPCs isolated from dog coronary arteries (A) and MPCs from the myocardium (B) formed multicellular clones. VPCs are c-kit (green) and flk1 (red) positive. MPCs are c-kit (green) positive and flk1-negative. C: Clonogenic VPCs differentiate into SMCs (α-SMA, green), 59-4%, ECs (vWf, yellow), 31±4%, and myocytes (α-SA, red), 10±2%. D: Clonogenic MPCs differentiate into SMCs, 16±6%, ECs, 11±5%, and myocytes, 73±9%.

FIG. 8. Translocation of PCs. Migrating EGFP-MPCs (A & B) are located within interstitial fibronectin tunnels (yellow). Arrows point to the direction of migration of the EGFP-MPCs established in living tissue by two-photon microscopy.

FIG. 9. PC translocation. A: Two-photon microscopy: 20 min after injection, EGFP-MPCs (green) are within the lumen of coronary vessels (red). B-F: Transcoronary migration of EGFP-MPCs; images of the same field were taken at 30 min intervals. Arrowheads point to 2 EGFP-MPCs detected in the living tissue. G: After fixation, migrated cells were identified by confocal microscopy. Myocytes are stained by cardiac myosin heavy chain (MHC: magenta).

FIG. 10. Position of the catheter (A, C) and injection of cardiac PCs together with Isopaque into the circumflex coronary artery (B) and the LAD (D) of a transplanted dog. Echocardiographic images of the transplanted heart at 8 (E) and 15 (F) days after surgery. (G) Isopaque and cell viability.

FIG. 11. Transplanted heart. A: The heart was cut in 22 slices and 114 sections were examined. B: Large transverse section of the LV in which a cluster of EGFP-positive (green) myocytes (α-sarcomeric actin, α-SA: red) is located in proximity of three areas of myocardial damage (MD). More than 2000 EGFP-positive cells are present. C: Four other examples of clusters of EGFP-positive myocytes within the transplanted heart. D: Newly formed EGFP-positive coronary vessels (EGFP: green; α-smooth muscle actin, α-SA: red). Inset: co-localization of EGFP and α-SMA in the vessel wall (yellow). E: Higher magnification of newly formed myocytes (left panels: EGFP, green; right panels: α-SA: red; arrows). F: EGFP-positive cells express GATA4 (red), Nkx2.5 (red) and GATA6 (red) documenting the acquisition of the myocyte and SMC lineage. G, H: Newly formed myocytes (α-SA, red) carry the Y-chr (white dots). I: By PCR, EGFP DNA sequences were detected only in the heart (H) but not in the kidney (K), spleen (S), lung (Lu) and liver (L). J: The recognition of Sry by PCR in the heart (H) indicates the presence of male cells of recipient origin in the donor heart. K, S, Lu and L correspond to organs of the recipient dog that have therefore a male genotype (SEQ ID NOS.: 3 and 4).

FIG. 12. BMPC differentiation and cell genotyping. A: Transgene constructs in donor mice. The promoter that controls the ubiquitous or myocyte restricted expression of the transgene is shown. Also the scheme illustrates that male donor BMPCs were injected intramyocardially in wild-type female infarcted mice. NLS, nuclear localization signal; MHC, myosin heavy chain; MI, myocardial infarct. Three classes of BMPCs were employed to induce myocardial regeneration: 1. Male EGFP-positive BMPCs from β-actin-EGFP mice; 2. Male EGFP-negative BMPCs from α-MHC-EGFP mice; and 3. Male EGFP-negative BMPCs from α-MHC-c-myc-tagged-nuc-Akt mice. B: In case 1, all cardiac cells generated by BMPC differentiation are expected to express EGFP; in case 2, only myocytes generated by BMPC differentiation are expected to express EGFP; and in case 3, only nuclei of myocytes generated by BMPC differentiation are expected to express c-myc-tag. C: The detection of the Y-chr allowed us to discriminate resident female cardiac cells from newly formed male cardiac cells generated by BMPC differentiation.

FIG. 13. A: BMPCs from α-MHC-c-myc-tagged-nuc-Akt mice regenerated myocytes (α-SA: red; c-myc: green; arrowheads). B: Infarcts treated with BMPCs from β-actin-EGFP mice. EP: epicardium; EN: endocardium. Left, central and right panels show EGFP (green), new myocytes (MHC, red) and their merge. Arrows: non regenerated infarct. C: Left, central and right panels illustrate new myocytes (MHC, red), distribution of Y-chr (white) and their merge. Arrows: non regenerated infarct. D: Higher magnification of new myocytes within the formed myocardium. The restored myocyte mass increased with time. E: DNA sequences (see SEQ ID NOS.: 5-10) of EGFP and c-myc-tag by PCR. DNA from the tail of donor TG and WT mice was employed as + and − control. F: Transcripts and sequences (see SEQ ID NOS.: 11-16) for EGFP and c-myc-tag by RT-PCR in infarcted treated hearts (+). Absence of RT reaction (−). RNA from hearts of TG and WT was employed as + and − control. G: EGFP and c-myc-tag protein by Western blotting.

FIG. 14. Lack of cell fusion. Regenerated human myocytes (A) and vessels (B) are Cre-recombinase positive (white) but EGFP-negative. C: Positive control: EGFP-myocytes of mice in which EGFP was driven by α-MHC promoter. D: Myocytes and vessels show at most two human X-chr (white dots; arrowheads). Mouse X-Chr (magenta dots; arrows) are present in myocytes bordering the infarct (BZ). See ref 139 for detail.

FIG. 15. PC engraftment. Male BMPCs (Y-chr: white dots) injected in the infarcted female mouse heart express N-cadherin (A: yellow) and connexin 43 (B: yellow). Connexin 43 and N-cadherin were detected between BMPCs and between BMPCs and resident myocytes (α-SA: red) and fibroblasts (procollagen: magenta). Apoptosis of BMPCs was restricted to non-engrafted cells (C); connexin 43 was absent in TdT labeled PCs (magenta). Engrafted BMPCs are BrdU-positive (D: yellow). Mitosis is shown by phospho-H3 labeling of metaphase chromosomes (E: yellow).

FIG. 16. A: A doppler flow transducer and hydraulic occluder were implanted on the LAD. A critical stenosis was created as shown by the absence of reactive hyperemia after release (R) of 15-sec occlusion. In the absence of stenosis (B), the release leads to reactive hyperemia shown as mean and phasic CBF in the upper and lower. C: Lack of reactive hyperemnia with critical stenosis 10 days after LAD constriction and the injection of EGFP-positive VPCs in six sites around the stenotic artery (A: red stars). As documented in D, 30 days after coronary constriction and cell implantation there was a slow return of CBF after release of 15-sec occlusion. These data suggest the formation of coronary vessels which restored in part CBF in the presence of a functional critical stenosis. Histologically, at 30 day, in proximity of the stenotic vessel, a large developing artery (E: diameter=˜1 mm) was identified (EGFP: green; α-SMA: red; arrowheads). Preexisting vessels are EGFP negative and α-SMA positive (arrows).

FIG. 17. AKANE protocol (Amplification of the Key DNA sequence Adjacent to an integrated provirus by Nested PCR coupled with Enzymatic digestion and ligation of the genome). This method corresponds to an inverse PCR which is the most sensitive strategy for the amplification of unknown DNA sequences that flank a region of known sequence. The primers are oriented in the reverse direction of the usual orientation and the template for the reverse primers is a restriction fragment that has been ligated and self-circularized. A: The AKANE method was first developed in human cardiac PCs infected with an EGFP lentivirus in vitro at low efficiency (˜10%). Genomic DNA was extracted, digested with EcoR1 and ligated with T4 DNA ligase to circularize the DNA fragments. Two sets of PCR primers were used to amrplify the coding region of the EGFP gene: (1) one set of conventional primers that produced a single band of 164 bp and (2) a set of primers with opposite directions that amplify only circularized DNA and produced a single band of 143 bp. B: To determine the clonal profile of the infected human cardiac PCs, extracted DNA was digested with Taq1, ligated with T4 DNA ligase and re-linearized with Hind3. One round of PCR and two additional nested PCR were perfbormed. The PCR primers employed in the first (1st) and second (2nd) amplification round were designed in the region of Long Terminal Repeat, LTR, which is commonly located at the 5′- and 3′-sides of the lentiviral genome. The PCR primers employed in the third round (3rd) were specific for either the 5′- or the 3′-side of the site of integration. In all cases, primers were oriented in the opposite direction. No clear bands were detected after the 1st round because of the low amount of the target templates in the sample. Arrows of the same color point to the corresponding bands in different lanes. As expected, the size of the amplicons decreased by 112 bp for the 5′-side products and 138 bp fob the 3′-side products. The seven bands indicated by the arrows reflect different sites of integration of the EGFP lentivirus in the genomic DNA of the infected human cardiac PCs. Two of the amplified bands were excised from the gel and the DNA was re-amplified as shown in the last two lanes. C: DNA sequencing analysis of the two re-amplified bands demonstrated that the DNA contained the proviral genome, shown in green, together with the key DNA sequence of the human genome, shown in blue. The human genome is linked to the proviral DNA through the integration site and the Taq1 restriction site. The sites of integration were located in chromosomes 20 and 6, respectively. D: Multiple clones were identified in human cardiac PCs, and the identified chromosomes are listed. E: After EGFP lentiviral infection (˜80% efficiency), human cardiac PCs were implanted in infarcted rats that were sacrificed one month later. Cardiac cells were enzymatically digested and separated in cardiac PCs, ECs, fibroblasts and myocytes. By the AKANE protocol, various clones were identified: one clone in c-kit positive cells, eight clones in ECs, four clones in fibroblasts, and six clones in myocytes. F: DNA sequencing analysis demonstrated that the DNA contained the proviral genome (green) together with the key DNA sequence of the human genome (blue). One of the detected clones was present in all committed cell types indicating that these cells constitute the progeny of one of the injected c-kit positive cardiac PCs which underwent multi lineage differentiation. G: An example of the detected sites of integration in the various cardiac cells of the same animal are listed. Some clones were common to different category of the cells (arrowheads). The distribution of the integration sites, again, confirmed the random integration of the EGFP lentivirus into the human genome.

FIG. 18. A: Angiogenesis corresponds to the sprouting of mature ECs and SMCs from pre-existing vessels. Therefore, the cells within the newly formed vessel will not express the reporter genes carried by the injected PCs. B: Vasculogenesis corresponds to sites of active neovascularization and is mediated by the recruitment of the delivered PCs. In this case, the cells in the regenerated vessels will express the reporter genes. C: Alternatively, Vasculogenesis corresponds to the recruitment of circulating EPCs and smooth muscle PCs (SMPCs), which together generate new vessels. In this case, the cells in the vessel wall will be negative for the reporter genes but will carry the Y-chr. DI: Adaptive arteriogenesis or collateral vessel formation corTesponds to the development of large vessels from pre-existing arteriolar anastomoses. Therefore, the cells within the wall of the collateral vessels will be negative for the reporter genes. E: Combination of angiogenesis and vasculogenesis may also occur resulting in the colocalization of cells negative and positive for the reporter genes within the wall of newly formed vessels.

FIG. 19. Physiology of newly generated myocytes. A: Contractility, action potential, calcium transients and voltage clamp currents in a small newly formed (left panel) and a large terminally differentiated (right panel) myocyte. Hypertrophied myocytes exhibit depressed contractility, which is paralleled by shorter action potential, decreased calcium transient and increased net outward current. B: Mechanical properties of myocytes generated by BMPCs injected in the infarcted mouse heart. Newly formed cells show green fluorescence, since BMPCs were obtained from transgenic mice expressing EGFP under the control of α-MHC promoter. Spared hypertrophied myocytes (phase contrast) are characterized by decreased fractional shortening. C: Membrane currents in myocytes generated by BMPCs. In comparison with surviving myocytes, new cells possess higher outward potassium current which, in turn, determines longer duration of the action potential.

DETAILED DESCRIPTION OF THE INVENTION

As used herein, “autologous” refers to something that is derived or transferred from the same individual's body (i.e., autologous blood donation; an autologous bone marrow transplant).

As used herein, “allogeneic” refers to something that is genetically different although belonging to or obtained from the same species (e.g., allogeneic tissue grafts or organ transplants).

As used herein, “stem cells” are used interchangeably with “progenitor cells” and refer to cells that have the ability to renew themselves through mitosis as well as differentiate into various specialized cell types. The stem cells used in the invention are somatic stem cells, such as bone marrow or cardiac stem cells or progenitor cells. “Vascular progenitor cells” or VPCs are a subset of adult cardiac stem cells that are c-kit positive and flk1 positive, which generate predominantly endothelial cells and smooth muscle cells. “Myocyte progenitor cells” or MPCs are a subset of adult cardiac stem cells that are c-kit positive and flk1 negative, which generate cardiomyocytes predominantly.

As used herein, “adult” stem cells refers to stem cells that are not embryonic in origin nor derived from embryos or fetal tissue.

Stem cells (e.g. progenitor cells) employed in the invention are advantageously selected to be lineage negative. The term “lineage negative” is known to one skilled in the art as meaning the cell does not express antigens characteristic of specific cell lineages. For example, bone marrow progenitor cells (BMPCs) do not express any of the hematopoietic lineage markers, such as CD3, CD20, CD33, CD14, and CD15. And, it is advantageous that the lineage negative stem cells are selected to be c-kit positive. The term “c-kit” is known to one skilled in the art as being a receptor which is known to be present on the surface of stem cells, and which is routinely utilized in the process of identifying and separating stem cells from other surrounding cells.

As used herein, the term “immunocompatible” refers to the antigenic similarity of cells or tissues from a donor source to the cells or tissues in a recipient subject such that the donor cells or tissues do not induce an immune response in the recipient subject. A donor cell or tissue that does not induce an immune response in a recipient and is not rejected by the recipient subject is said to be immunocompatible.

As used herein, the term “cytokine” is used interchangeably with “growth factor” and refers to peptides or proteins that bind receptors on cell surfaces and initiate signaling cascades thus influencing cellular processes. The terms “cytokine” and “growth factor” encompass functional variants of the native cytokine or growth factor. A functional variant of the cytokine or growth factor would retain the ability to activate its corresponding receptor. Variants can include amino acid substitutions, insertions, deletions, alternative splice variants, or fragments of the native protein. The term “variant” with respect to a polypeptide refers to an amino acid sequence that is altered by one or more amino acids with respect to a reference sequence. The variant can have “conservative” changes, wherein a substituted amino acid has similar structural or chemical properties, e.g., replacement of leucine with isoleucine. Alternatively, a variant can have “nonconservative” changes, e.g., replacement of a glycine with a tryptophan. Analogous minor variations can also include amino acid deletion or insertion, or both. Guidance in determining which amino acid residues can be substituted, inserted, or deleted without eliminating biological activity can be found using computer programs well known in the art, for example, DNASTAR software.

As used herein, “patient” or “subject” may encompass any vertebrate including but not limited to humans, mammals, reptiles, amphibians and fish. However, advantageously, the patient or subject is a mammal such as a human, or a mammal such as a domesticated mammal, e.g., dog, cat, horse, and the like, or production mammal, e.g., cow, sheep, pig, and the like.

The pharmaceutical compositions of the present invention may be used as therapeutic agents—i.e. in therapy applications. As herein, the terms “treatment” and “therapy” include curative effects, alleviation effects, and prophylactic effects. In certain embodiments, a therapeutically effective dose of progenitor cells is applied, delivered, or administered to the heart or implanted into the heart. An effective dose or amount is an amount sufficient to effect a beneficial or desired clinical result. Said dose could be administered in one or more administrations.

Mention is made of the following related pending patent applications:

U.S. Application Publication No. 2003/0054973, filed Jun. 5, 2002, which is herein incorporated by reference in its entirety, discloses methods, compositions, and kits for repairing damaged myocardium and/or myocardial cells including the administration of cytokines.

U.S. Application Publication No. 2006/0239983, filed Feb. 16, 2006, which is herein incorporated by reference in its entirety, discloses methods, compositions, and kits for repairing damaged myocardium and/or myocardial cells including the administration of cytokines and/or adult stem cells as well as methods and compositions for the development of large arteries and vessels. The application also discloses methods and media for the growth, expansion, and activation of human cardiac stem cells.

Successful transplantation has an inherent yearly 6% mortality and most patients die within 10-12 years. The improved immunosuppressive regimen has resulted in increased short-term survival but long-term survival has remained largely the same. Post-operative morbidity and mortality associated with cardiac transplantation is dictated by acute and chronic complications which rapidly affect the performance of the new heart or lead with time to a progressive deterioration of cardiac function. Chronic rejection with accelerated cardiac allograft vasculopathy (CAV) is the major pathological event that determines the fatal evolution of the transplanted heart. Graft failure due to CAV is characterized by occlusive vessel disease that results in myocardial infarction, multiple focal areas of tissue injury, arrhythmias, sudden death and congestive heart failure. Infarct healing with scar formation is impaired by immunosuppressive therapy which further complicates the devastating consequences of graft atherosclerosis and arteriosclerosis. The mechanisms of graft atherosclerosis and arteriosclerosis are not understood but repetitive cell-mediated and/or humoral-mediated immunological damage followed by a potentiated myointimal response are involved in the manifestations of this unique form of coronary artery disease. Thus, three interrelated pathologic processes appear to be critical determinants of heart failure in the transplanted heart: rejection, evolving coronary atherosclerosis and chronic ischemic myocardial injury.

Chronic rejection with accelerated graft atherosclerosis is the major pathological event that determines the fatal evolution of the transplanted heart. Occlusive vessel disease of the large, intermediate and small coronary arteries results in multiple focal areas of injury, myocardial infarction and ischemic heart failure. The novel methods of the invention provide a solution to the major problems associated with the unfavorable progression of cardiac transplantation in humans by employing progenitor cells from the recipient to repopulate the donor heart with immunocompatible cardiomyocytes and coronary vessels.

Functionally competent cardiac progenitor cells also known as cardiac stem cells are present in the explanted heart of patients undergoing cardiac transplantation and these can be isolated and grown in vitro for subsequent autologous cell therapy. Additionally, in the acute phase, bone marrow progenitor cells (BMPCs) from the recipient can be utilized in view of their ability to transdifferentiate and acquire the cardiomyocyte fate and form vascular structures.

Thus, the donor heart can provide the scaffolding for the generation of a new heart derived from implantation, engraftment and differentiation of BMPCs and cardiac progenitor cells isolated from the recipient. Two distinct classes of cardiac progenitor cells exist within the heart: vascular progenitor cells (VPCs) and myocyte progenitor cells (MNPCs). VPCs are programmed to differentiate predominantly into vascular smooth muscle cells (SMCs) and endothelial cells (ECs), but also have the ability to acquire the cardiomyocyte lineage. On the other hand, MPCs predominantly generate cardiomyocytes and to a more limited extent SMCs and ECs.

Successful engraftment of progenitor cells is the initial process of tissue repair. Myocardial reconstitution necessitates the generation of a cardiomyocyte compartment together with a proportional coronary vasculature. Myocytes alone in the absence of adequate blood supply cannot perform their function, and coronary vessels alone without muscle mass cannot restore cardiac performance (36, 184, 185). Engrafted progenitor cells may result in a coordinated growth response in which myocytes and vessels are concurrently formed to engender functionally competent myocardium. Coronary blood flow is regulated by conductive coronary arteries and resistance coronary arterioles (186) while oxygen availability and diffusion are controlled by the capillary network (136, 188).

BMPCs, VPCs, and MPCs isolated from the recipient can be delivered to the donor heart to promote the formation of immunocompatible myocardium within the non-immunocompatible transplanted heart. The reconstituted myocardium will be comprised of immunocompatible coronary vessels and coronary myocytes which can replace and/or repair the non-immunocompatible diseased arteries and myocardium. Thus, immunosuppressive therapy may no longer be required resulting in significant improvement of quality of life and lifespan of patients after cardiac transplantation.

The present invention provides methods of reducing transplant rejection in a subject by isolating cardiac or bone marrow progenitor cells from tissue specimens from the recipient, expanding and optionally activating the progenitor cells in culture, and subsequently administering the recipient's progenitor cells to the transplanted donor heart. The implanted progenitor cells then generate immunocompatible endothelial cells, smooth muscle cells, and cardiomyocytes within the non-immunocompatible donor myocardium, which assemble into immunocompatible myocardium and myocardial vessels, thus reducing the immune response to the donor organ.

In one embodiment, the present invention provides a method of reducing an immune response to a transplanted donor heart in a subject comprising obtaining myocardial tissue from the subject's explanted heart; extracting cardiac progenitor cells from said myocardial tissue; expanding said cardiac progenitor cells in culture; and administering said cardiac progenitor cells to the transplanted donor heart, wherein said cardiac progenitor cells generate immunocompatible myocardium and immunocompatible myocardial vessels following their administration, thereby reducing the immune response to said transplanted donor heart. In some embodiments, the subject is human.

It is preferable that the cardiac progenitor cells be c-kit positive. The c-kit stem cell marker is associated with progenitor cells with apparent comparable functional behavior for cardiac repair whether they derive from the heart or the bone marrow (47, 48, 51, 57, 59, 64, 139, 140). In some embodiments, the cardiac progenitor cells are separated into vascular progenitor cells and myocyte progenitor cells prior to administration. Recently, the inventors have discovered that the adult heart in mice, dogs and humans contains two populations of progenitor cells (PCs); a vascular progenitor cell (VPC), which is stored in niches located within the wall of coronary vessels, and a myocyte progenitor cell (MPC), which is located in myocardial niches, distinct from vascular niches (FIG. 5). See also U.S. Provisional Application No. 60/991,515, which is herein incorporated by reference in its entirety. VPCs are primitive cells which are self-renewing, clonogenic and multipotent in vitro and can regenerate coronary vessels in vivo. Although coronary VPCs are programmed to differentiate predominantly into smooth muscle cells (SMCs) and endothelial cells (ECs), they also possess the inherent ability to acquire modestly the cardiomyocyte lineage. Conversely, MPCs generate predominantly cardiomyocytes and to a limited extent vascular SMCs and ECs.

The c-kit marker is present in the absence of flk1 in MPCs (29, 64, 138-140) and together with flk1 in VPCs (FIG. 5). Therefore, the pool of lineage negative c-kit-positive PCs in the heart may be separated into two cell categories according to the expression of the vascular endothelial growth factor receptor 2 (VEGF-R2/flk1). The expression of VEGFR2 or kinase domain receptor (KDR/flk1), which represents the earliest marker of angioblast precursors (141-145), is a good predictor of VPCs. Flk1 is an epicardium-specific marker and epicardial-derived cells initiate vasculogenesis in the prenatal heart (146, 147). In the mouse embryo, flk1 is necessary for the development of the coronary vasculature (148, 149). Recent results have suggested that the growth potential of flk1-positive PCs exceeds hematopoiesis and vasculogenesis (144, 145, 150-156). The endocardium and a small population of cells in the myocardium originate from a pool of flk1-positive cells (153-156). Additionally, multipotent flk1 PCs form colonies of ECs, SMCs and myocytes (145). Thus, the expression of flk1 and c-kit may be utilized to distinguish VPCs and MPCs. In one embodiment, the vascular progenitor cells are c-kit positive and flk1 positive. In another embodiment, the vascular progenitor cells differentiate into immunocompatible endothelial cells and smooth muscle cells. In another embodiment, the myocyte progenitor cells are c-kit positive and flk1 negative. In still another embodiment, the myocyte progenitor cells differentiate into immunocompatible cardiomyocytes.

In another embodiment, the present invention provides a method of reducing an immune response to a transplanted donor heart in a subject comprising obtaining myocardial tissue from the subject's explanted heart; extracting cardiac myocyte progenitor cells from said myocardial tissue; expanding said myocyte progenitor cells in culture; and administering said myocyte progenitor cells to the transplanted donor heart, wherein said myocyte progenitor cells generate immunocompatible myocardium following their administration, thereby reducing the immune response to said transplanted donor heart. In some embodiments, the myocyte progenitor cells are c-kit positive and flk1 negative. In other embodiments the myocyte progenitor cells differentiate into immunocompatible cardiomyocytes.

Adult bone marrow progenitor cells (BMPCs) are capable of generating mature cells beyond their own tissue boundaries, a process which has been termed developmental plasticity. Based on this premise, the inventors have documented that BMPCs regenerate infarcted myocardium in rodents leading to the formation of cardiomyocytes and coronary vessels which are structurally and functionally connected to resident cardiomyocytes and the primary coronary circulation. Thus, BMPCs can also be employed to generate immunocompatible myocardium to prevent rejection of a transplanted heart. Because BMPCs can be obtained from the recipient subject prior to the transplant surgery, the BMPCs can be expanded in culture and ready for administration to the donor heart at the time of the transplant surgery. Therefore, in another embodiment of the invention, the method of reducing an immune response to a transplanted donor heart in a subject comprises obtaining a bone marrow specimen from the subject; extracting adult bone marrow progenitor cells from said specimen; expanding said bone marrow progenitor cells in culture; and administering said bone marrow progenitor cells to the transplanted donor heart, wherein said bone marrow progenitor cells generate immunocompatible myocardium and immunocompatible myocardial vessels following their administration, thereby reducing the immune response to said transplanted donor heart. In some embodiments, the bone marrow progenitor cells are administered immediately after transplantation.

The stem cell antigen c-kit is expressed in a population of BMPCs that are capable of differentiating into cardiomyocytes and SMCs and ECs organized in coronary vessels (47, 48, 51). Therefore, the presence of c-kit may be employed to isolate BMPCs. Accordingly, in one embodiment of the invention, the bone marrow progenitor cells are c-kit positive. In another embodiment, the bone marrow progenitor cells differentiate into immunocompatible endothelial cells, smooth muscle cells, and cardiomyocytes.

In another embodiment, vascular progenitor cells and/or myocyte progenitor cells may be administered to the donor heart following administration of bone marrow progenitor cells. For instance, in some embodiments, the method further comprises extracting cardiac progenitor cells from said subject's explanted heart; separating said cardiac progenitor cells into vascular progenitor cells and myocyte progenitor cells; and administering said vascular progenitor cells and myocyte progenitor cells to the transplanted donor heart. In such embodiments, the BMPCs administered at the time of transplant surgery initiate the generation of immunocompatible myocardial tissue and vessels, and this generation is expanded by the subsequent administration of VPCs and MPCs. The VPCs and MPCs may be administered multiple times after transplantation and the multiple administrations may occur at a set interval after the administration of the BMPCs. For example, VPCs and/or MPCs may be administered to the donor heart every week, two weeks, three weeks, month, two months, three months, six months, nine months, year, two years, three years, or five years after BMPC administration.

The present invention also provides a method of reducing cardiac allograft vasculopathy in a subject who has received a transplanted donor heart. Cardiac allograft vasculopathy is an accelerated form of coronary artery disease that affects the vasculature of the allograft and is the primary cause of death in transplant patients surviving one year after transplantation. The non-immunocompatible tissue of the allograft induces an immune response in the recipient subject that leads to endothelial cell damage and vascular injury. The vascular injury initiates a repair response that can lead to the occlusion of the vessel and subsequent infarction.

Use of cardiac progenitor cells isolated from the recipient may be used to generate immunocompatible myocardial tissue in the donor heart to reduce an immune response, and thus also reduce the development of cardiac allograft vasculopathy. In addition, vascular progenitor cells obtained from the recipient subject can be employed to generate immunocompatible vessels in the donor heart that would not be susceptible to immune-mediated injury. Thus, in one embodiment of the invention, the method of reducing cardiac allograft vasculopathy in a subject comprises obtaining myocardial tissue from the subject's explanted heart; extracting cardiac vascular progenitor cells from said myocardial tissue; expanding said vascular progenitor cells in culture; and administering said vascular progenitor cells to the transplanted donor heart, wherein said vascular progenitor cells generate immunocompatible coronary vasculature, thereby repairing/and or regenerating the non-immunocompatible coronary arteries of the donor heart. In some embodiments, the vascular progenitor cells are c-kit positive and flk1 positive. In other embodiments, the vascular progenitor cells differentiate into immunocompatible endothelial cells and smooth muscle cells.

Progenitor cells may be isolated from tissue specimens, such as myocardium or bone marrow, obtained from a subject or patient, such as the transplant recipient. By way of example, myocardial tissue specimens obtained from the recipient's explanted heart may be minced and placed in appropriate culture medium. Cardiac progenitor cells growing out from the tissue specimens can be observed in approximately 1-2 weeks after initial culture. At approximately 4 weeks after the initial culture, the expanded progenitor cells may be collected by centrifugation. An exemplary method for obtaining bone marrow progenitor cells from a subject is described as follows. Bone marrow may be harvested from the iliac crests using a needle and the red blood cells in the sample may be lysed using standard reagents. Bone marrow progenitor cells are collected from the sample by density gradient centrifugation. Optionally, the bone marrow progenitor cells may be expanded in culture. Other methods of isolating adult progenitor cells, such as bone marrow progenitor cells and cardiac progenitor cells, from a subject are known in the art and can be employed to obtain suitable progenitor cells for use in the methods of the invention. U.S. Patent Application Publication No. 2006/0239983, filed Feb. 16, 2006, which is herein incorporated by reference in its entirety, describes media appropriate for culturing and expanding adult progenitor cells. However, one of ordinary skill in the art would be able to determine the necessary components and modify commonly used cell culture media to be employed in culturing the isolated progenitor cells of the invention.

It is preferable that the progenitor cells of the invention are lineage negative. Lineage negative progenitor cells can be isolated by various means, including but not limited to, removing lineage positive cells by contacting the progenitor cell population with antibodies against lineage markers and subsequently isolating the antibody-bound cells by using an anti-immunoglobulin antibody conjugated to magnetic beads and a biomagnet. Alternatively, the antibody-bound lineage positive stem cells may be retained on a column containing beads conjugated to anti-immunoglobulin antibodies. For instance, lineage negative bone marrow progenitor cells may be obtained by incubating mononuclear cells isolated from a bone marrow specimen with immunomagnetic beads conjugated with monoclonal antibodies for CD13 (T lymphocytes), CD20 (B lymphocytes), CD33 (myeloid progenitors), CD14 and CD15 (monocytes). The cells not bound to the immunomagnetic beads represent the lineage negative bone marrow progenitor cell fraction and may be isolated. Similarly, cells expressing markers of the cardiac lineage may be removed from cardiac progenitor cell populations to isolate lineage negative cardiac progenitor cells.

In a preferred embodiment of the invention, the lineage negative progenitor cells express the stem cell surface marker, c-kit, which is the receptor for stem cell factor. Positive selection methods for isolating a population of lineage negative progenitor cells expressing c-kit are well known to the skilled artisan. Examples of possible methods include, but are not limited to, various types of cell sorting, such as fluorescence activated cell sorting (FACS) and magnetic cell sorting as well as modified forms of affinity chromatography. In a preferred embodiment, the lineage negative progenitor cells are c-kit positive. In some embodiments, c-kit positive cardiac progenitor cells are further separated into subpopulations of cells expressing the VEGFR2 receptor, flk1. Cardiac progenitor cells that are c-kit positive and flk1 positive are vascular progenitor cells, while cardiac progenitor cells that are c-kit positive and flk1 negative are myocyte progenitor cells. Similar positive selection methods for isolating c-kit positive progenitor cells may be used to select cells expressing the flk1 receptor (e.g. immunobeads, cell sorting, affinity chromatography, etc.).

Isolated lineage negative, c-kit positive progenitor cells may be plated individually in single wells of a cell culture plate and expanded to obtain clones from individual progenitor cells. In some embodiments, cardiac progenitor cells that are c-kit positive and flk1 positive are plated individually to obtain pure cultures of vascular progenitor cells. In other embodiments, cardiac progenitor cells that are c-kit positive and flk1 negative are plated individually to obtain pure cultures of myocyte progenitor cells.

In certain embodiments of the invention, the cardiac progenitor cells or bone marrow progenitor cells are activated prior to administration. Activation of the progenitor cells may be accomplished by exposing the progenitor cells to one or more cytokines. Suitable concentrations of the one or more cytokines for activating the progenitor cells include a concentration of about 0.1 to about 500 ng/ml, about 10 to about 500 ng/ml, about 20 to about 400 ng/ml, about 30 to about 300 ng/ml, about 50 to about 200 ng/ml, or about 80 to about 150 ng/ml. In one embodiment, the concentration of one or more cytokines is about 25, about 50, about 75, about 100, about 125, about 150, about 175, about 200, about 225, about 250, about 275, about 300, about 325, about 350, about 375, about 400, about 425, about 450, about 475, or about 500 ng/ml. In some embodiments, the cardiac progenitor cells or bone marrow progenitor cells are activated by contact with hepatocyte growth factor (HGF), insulin-like growth factor-1 (IGF-1), or variant thereof.

HGF positively influences stem cell migration and homing through the activation of the c-Met receptor (Kollet et al. (2003) J. Clin. Invest. 112: 160-169; Linke et al. (2005) Proc. Natl. Acad. Sci. USA 102: 8966-8971; Ros-Myles et al. (2005) J. Cell. Sci. 118: 4343-4352; Urbanek et al. (2005) Circ. Res. 97: 663-673). Similarly, IGF-1 and its corresponding receptor (IGF-IR) induce cardiac stem cell division, upregulate telomerase activity, hinder replicative senescence and preserve the pool of functionally-competent cardiac stem cells in the heart (Kajstura et al. (2001) Diabetes 50: 1414-1424; Torella et al. (2004) Circ. Res. 94: 514-524; Davis et al. (2006) Proc. Natl. Acad. Sci. USA 103: 8155-8160). In some embodiments, the cardiac progenitor cells or bone marrow progenitor cells are contacted with HGF and IGF-1.

Some other non-limiting examples of cytokines that are suitable for the activation of the cardiac progenitor cells or bone marrow progenitor cells include Activin A, Bone Morphogenic Protein 2, Bone Morphogenic Protein 4, Bone Morphogenic Protein 6, Cardiotrophin-1, Fibroblast Growth Factor 1, Fibroblast Growth Factor 4, Flt3 Ligand, Glial-Derived Neurotrophic Factor, Heparin, Insulin-like Growth Factor-II, Insulin-Like Growth Factor Binding Protein-3, Insulin-Like Growth Factor Binding Protein-5, Interleukin-3, Interleukin-6, Interleukin-8, Leukemia Inhibitory Factor, Midkine, Platelet-Derived Growth Factor AA, Platelet-Derived Growth Factor BB, Progesterone, Putrescine, Stem Cell Factor, Stromal-Derived Factor-1, Thrombopoietin, Transforming Growth Factor-α, Transforming Growth Factor-β1, Transforming Growth Factor-β2, Transforming Growth Factor-□β3, Vascular Endothelial Growth Factor, Wnt1, Wnt3a, and Wnt5a, as described in Kanemura et al. (2005) Cell Transplant. 14:673-682; Kaplan et al. (2005) Nature 438:750-751; Xu et al. (2005) Methods Mol. Med. 121:189-202; Quinn et al. (2005) Methods Mol. Med. 121:125-148; Almeida et al. (2005) J Biol Chem. 280:41342-41351; Barnabe-Heider et al. (2005) Neuron 48:253-265; Madlambayan et al. (2005) Exp Hematol 33:1229-1239; Kamanga-Sollo et al. (2005) Exp Cell Res 311:167-176; Heese et al. (2005) Neuro-oncol. 7:476-484; He et al. (2005) Am J Physiol. 289:H968-H972; Beattie et al. (2005) Stem Cells 23:489-495; Sekiya et al. (2005) Cell Tissue Res 320:269-276; Weidt (2004) Stem Cells 22:890-896; Encabo et al (2004) Stem Cells 22:725-740; and Buytaeri-Hoefen et al. (2004) Stem Cells 22:669-674, the entire text of each of which is incorporated herein by reference.

Functional variants of the above-mentioned cytokines can also be employed in the invention. Functional cytokine variants would retain the ability to bind and activate their corresponding receptors. Variants can include amino acid substitutions, insertions, deletions, alternative splice variants, or fragments of the native protein. For example, NK1 and NK2 are natural splice variants of HGF, which are able to bind to the c-MET receptor. These types of naturally occurring splice variants as well as engineered variants of the cytokine proteins that retain function can be employed to activate the progenitor cells of the invention.

The present invention involves administering a therapeutically effective dose or amount of progenitor cells to a donor heart. An effective dose is an amount sufficient to effect a beneficial or desired clinical result. Said dose could be administered in one or more administrations. In some embodiments, at least three effective doses are administered to the donor heart in the recipient subject. In other embodiments, at least five effective doses are administered to the donor heart in the recipient subject. Each administration of progenitor cells may comprise a single type of progenitor cell (e.g. BMPC, VPC, or MPC) or may contain mixtures of the different types of progenitor cells. In one embodiment, bone marrow progenitor cells (BMPCs) are administered to the subject at the time of transplantation, and vascular progenitor cells (VPCs) and/or myocyte progenitor cells (MPCs) are administered at set intervals after transplantation. Examples of suitable intervals include, but are not limited to, 1 week, 2 weeks, 3 weeks, 1 month, 2 months, 3 months, 6 months, 12 months, 18 months or 24 months.

An effective dose of progenitor cells may be from about 2×10⁴ to about 1×10⁷, more preferably about 1×10⁵ to about 6×10⁶, or most preferably about 2×10⁶. As illustrated in the examples, 2×10⁶ to 1×10⁷ progenitor cells are used to effect regeneration of immunocompatible myocardium in a canine model. Although there would be a size difference between the heart of a canine and the heart of a human, it is likely that this range of progenitor cells would be sufficient in a human as well. However, the precise determination of what would be considered an effective dose may be based on factors individual to each patient, including their size, age, size of donor heart, type of repopulating progenitor cells (e.g. VPCs, MPCs, or BMPCs), and amount of time after transplantation. One ski lied in the art, specifically a physician or cardiologist, would be able to determine the number of progenitor cells that would constitute an effective dose without undue experimentation.

The progenitor cells (e.g. stem cells) may be administered to the heart by injection. The injection is preferably intramyocardial. As one skilled in the art would be aware, this is the preferred method of delivery for stem cells as the heart is a functioning muscle. Injection by this route ensures that the injected material will not be lost due to the contracting movements of the heart.

In another embodiment, the progenitor cells are administered by injection transendocardially or trans-epicardially. In another embodiment of the invention, the progenitor cells are administered using a catheter-based approach to deliver the trans-endocardial injection. The use of a catheter precludes more invasive methods of delivery wherein the opening of the chest cavity would be necessitated. As one skilled in the art would appreciate, optimum time of recovery would be allowed by the more minimally invasive procedure. A catheter approach involves the use of such techniques as the NOGA catheter or similar systems. The NOGA catheter system facilitates guided administration by providing electromechanic mapping of the area of interest, as well as a retractable needle that can be used to deliver targeted injections or to bathe a targeted area with a therapeutic. Any of the embodiments of the present invention can be administered through the use of such a system to deliver injections or provide a therapeutic. One of skill in the art will recognize alternate systems that also provide the ability to provide targeted treatment through the integration of imaging and a catheter delivery system that can be used with the present invention. Information regarding the use of NOGA and similar systems can be found in, for example, Sherman (2003) Basic Appl. Myol. 13: 11-14; Patel et al. (2005) The Journal of Thoracic and Cardiovascular Surgery 130:1631-38; and Perrin et al. (2003) Circulation 107: 2294-2302; the text of each of which are incorporated herein in their entirety.

In still another embodiment, the progenitor cells may be administered to a donor heart by an intracoronary route. This route obviates the need to open the chest cavity to deliver the cells directly to the heart. One of skill in the art will recognize other useful methods of delivery or implantation which can be utilized with the present invention, including those described in Dawn et al. (2005) Proc. Natl. Acad. Sci. USA 102, 3766-3771, the contents of which are incorporated herein in their entirety.

In some embodiments, the methods of the invention described herein further comprise administering to the subject an immunosuppressive therapy or imnmunosuppressant. Non-limiting examples of immunosuppressants include cyclosporine A, azathioprine, glucocorticoids (e.g. methylprednisolone, cortisol, prednisone, dexamethasone, betamethasone), cyclophosphamide, methotrexate, mercaptopurine, dactinomycin, anthracyclines, mitomycin C, bleomycin, mithramycin, tacrolimus, sirolimus, everolimus, myriocin, and antibodies (e.g. basiliximab, daclizumab, anti-thymocyte globulin, anti-lymphocyte globulin). Other therapeutic agents that are typically given to transplant patients, for instance HMG-CoA reductase inhibitors, rapamycin, and paclitaxel, may also be used in combination with the administration of progenitor cells. The immunosuppressants or other therapeutic agents may be administered to the subject in multiple doses subsequent to the administration of the progenitor cells. The immunosuppressants or other therapeutic agents may be taken on a routine schedule for a set period of time. For example, the immunosuppressants or other therapeutic agents may be taken once daily for about 1 month, about 2 months, about 3 months, about 6 months, about 12 months, or about 24 months after transplantation and administration of the progenitor cells. Other dosing schedules may be employed. Preferably, the dose and/or frequency of immunosuppressants or other therapeutic agents will be reduced following one or more administrations of the progenitor cells to the donor heart. One of skill in the art, particularly a physician or cardiologist, would be able to determine the appropriate dose and schedule for the administration of the immunosuppressants or other therapeutic agents.

The invention also comprehends methods for preparing compositions, such as pharmaceutical compositions, including one or more of the different type of progenitor cells described herein, for instance, for use in inventive methods for reducing cardiac allograft vasculopathy or transplant rejection. In one embodiment, the pharmaceutical composition comprises bone marrow progenitor cells and a pharmaceutically acceptable carrier, wherein said bone marrow progenitor cells are c-kit positive. In another embodiment, the pharmaceutical composition comprises vascular progenitor cells and a pharmaceutically acceptable carrier, wherein said vascular progenitor cells are c-kit positive and flk1 positive. In another embodiment, the pharmaceutical composition comprises myocyte progenitor cells and a pharmaceutically acceptable carrier, wherein said myocyte progenitor cells are c-kit positive and flk1 negative. In still another embodiment, the pharmaceutical composition comprises vascular progenitor cells, myocyte progenitor cells and a pharmaceutically acceptable carrier, wherein said vascular progenitor cells are c-kit positive and flk1 positive and said myocyte progenitor cells are c-kit positive and flk1 negative.

In an additionally preferred aspect, the pharmaceutical compositions of the present invention are delivered via injection. These routes for administration (delivery) include, but are not limited to, subcutaneous or parenteral including intravenous, intraarterial (e.g. intracoronary), intramuscular, intraperitoneal, intramyocardial, transendocardial, trans-epicardial, intranasal administration as well as intrathecal, and infusion techniques. Accordingly, the pharmaceutical composition is preferably in a form that is suitable for injection.

When administering a therapeutic of the present invention parenterally, it will generally be formulated in a unit dosage injectable form (solution, suspension, emulsion). The pharmaceutical formulations suitable for injection include sterile aqueous solutions or dispersions and sterile powders for reconstitution into sterile injectable solutions or dispersions. The carrier can be a solvent or dispersing medium containing, for example, water, ethanol, polyol (for example, glycerol, propylene glycol, liquid polyethylene glycol, and the like), suitable mixtures thereof and vegetable oils.

Proper fluidity can be maintained, for example, by the use of a coating such as lecithin, by the maintenance of the required particle size in the case of dispersion, and by the use of surfactants. Nonaqueous vehicles such a cottonseed oil, sesame oil, olive oil, soybean oil, corn oil, sunflower oil, or peanut oil and esters, such as isopropyl myristate, may also be used as solvent systems for compound compositions.

Additionally, various additives which enhance the stability, sterility, and isotonicity of the compositions, including antimicrobial preservatives, antioxidants, chelating agents, and buffers, can be added. Prevention of the action of microorganisms can be ensured by various antibacterial and antifungal agents, for example, parabens, chlorobutanol, phenol, sorbic acid, and the like. In many cases, it will be desirable to include isotonic agents, for example, sugars, sodium chloride, and the like. Prolonged absorption of the injectable pharmaceutical form can be brought about by the use of agents delaying absorption, for example, aluminum monostearate and gelatin. According to the present invention, however, any vehicle, diluent, or additive used would have to be compatible with the progenitor cells and other compounds used in combination with the progenitor cells.

Sterile injectable solutions can be prepared by incorporating the compounds utilized in practicing the present invention in the required amount of the appropriate solvent with various amounts of the other ingredients, as desired.

The pharmaceutical compositions of the present invention, e.g., comprising a therapeutic dose of progenitor cells (e.g. BMAPCs, VPC, and MPCs), can be administered to the patient in an injectable formulation containing any compatible carrier, such as various vehicles, adjuvants, additives, and diluents. Compounds, such as immunosuppressants or other therapeutic agents, to be administered as a combination therapy with the progenitor cells can be administered parenterally to the patient in the form of slow-release subcutaneous implants or targeted delivery systems such as monoclonal antibodies, iontophoretic, polymer matrices, liposomes, and microspheres.

Examples of compositions comprising a therapeutic of the invention include liquid preparations for parenteral, subcutaneous, intradermal, intramuscular, intracoronarial, intramyocardial or intravenous administration (e.g., injectable administration), such as sterile suspensions or emulsions. Such compositions may be in admixture with a suitable carrier, diluent, or excipient such as sterile water, physiological saline, glucose or the like. The compositions can also be lyophilized. The compositions can contain auxiliary substances such as wetting or emulsifying agents, pH buffering agents, gelling or viscosity enhancing additives, preservatives, flavoring agents, colors, and the like, depending upon the route of administration and the preparation desired. Standard texts, such as “REMINGTON'S PHARMACEUTICAL SCIENCE”, 17th edition, 1985, incorporated herein by reference, may be consulted to prepare suitable preparations, without undue experimentation.

The compositions can be isotonic, i.e., they can have the same osmotic pressure as blood and lacrimal fluid. The desired isotonicity of the compositions of this invention may be accomplished using sodium chloride, or other pharmaceutically acceptable agents such as dextrose, boric acid, sodium tartrate, propylene glycol or other inorganic or organic solutes. Sodium chloride is preferred particularly for buffers containing sodium ions.

Viscosity of the compositions may be maintained at the selected level using a pharmaceutically acceptable thickening agent. Methylcellulose is preferred because it is readily and economically available and is easy to work with. Other suitable thickening agents include, for example, xanthan gum, carboxymethyl cellulose, hydroxypropyl cellulose, carbomer, and the like. The preferred concentration of the thickener will depend upon the agent selected. The important point is to use an amount which will achieve the selected viscosity. Viscous compositions are normally prepared from solutions by the addition of such thickening agents.

A pharmaceutically acceptable preservative can be employed to increase the shelf-life of the compositions. Benzyl alcohol may be suitable, although a variety of preservatives including, for example, parabens, thimerosal, chlorobutanol, or benzalkonium chloride may also be employed. A suitable concentration of the preservative will be from 0.02% to 2% based on the total weight although there may be appreciable variation depending upon the agent selected.

Those skilled in the art will recognize that the components of the compositions should be selected to be chemically inert with respect to the active compound. This will present no problem to those skilled in chemical and pharmaceutical principles, or problems can be readily avoided by reference to standard texts or by simple experiments (not involving undue experimentation), from this disclosure and the documents cited herein.

The inventive compositions of this invention are prepared by mixing the ingredients following generally accepted procedures. For example, isolated progenitor cells can be resuspended in an appropriate pharmaceutically acceptable carrier and the mixture adjusted to the final concentration and viscosity by the addition of water or thickening agent and possibly a buffer to control pH or an additional solute to control tonicity. Generally the pH may be from about 3 to 7.5. Compositions can be administered in dosages and by techniques well known to those skilled in the medical and veterinary arts taking into consideration such factors as the age, sex, weight, and condition of the particular patient, and the composition form used for administration (e.g., liquid). Dosages for humans or other mammals can be determined without undue experimentation by the skilled artisan, from this disclosure, the documents cited herein, and the knowledge in the art.

Suitable regimes for initial administration and further doses or for sequential administrations also are variable, may include an initial administration followed by subsequent administrations; but nonetheless, may be ascertained by the skilled artisan, from this disclosure, the documents cited herein, and the knowledge in the art.

This invention is further illustrated by the following additional examples that should not be construed as limiting. The contents of all references, patents and published patent applications cited throughout this application, as well as the Figures, are incorporated herein by reference in their entirety.

EXAMPLES Example 1 Cardiac Transplantation in Dogs

In all examples described herein, female dog hearts are transplanted in male dogs and the cells to be injected (bone marrow progenitor cells (BMPCs), vascular progenitor cells (VPCs) or myocyte progenitor cells (MPCs)) are infected with a lentivirus expressing enhanced green fluorescent protein (EGFP), β-gal or red fluorescent protein (RFP) so that the progeny formed by cells given at different time points can be identified and measured.

In the last two years, a tremendous effort was made to develop a model of cardiac transplantation in the dog. The dog model was chosen after careful review because the dog is the smallest animal that fits the experimental requirements. Immunosuppression is well described in dogs (198-200) and canine MPCs and VPCs (64; FIGS. 5-7) have been isolated, expanded and characterized in vitro and in vivo. Thus, the use of the dog model maximizes efficiency.

In addition, data in the transplanted dog heart model show inflammatory infiltrates in the major coronary vessels and distal branches together with initial myointimal thickening (FIG. 4). Additionally, vast zones of damage characterized by clusters of T′ lymphocytes, monocytes and macrophages have been detected in the ventricular myocardium. Typically, myocytes are lost and collagen accumulates in the areas of injury. Of the 113 samples examined in this case myocardial pathology was identified in 90. These results indicate that the transplanted dog heart is a good model of cardiac allograft vasculopathy which occurs in human cardiac transplants.

A. Surgery

The female donor dog is positioned, heparin, 300 IU/kg, administered and anesthesia induced by thiopental, 6-10 mg/kg. A left lateral thoracotomy is performed, the pericardium opened, cardioplegic solution (ViaSpan) infused and the heart explanted and kept on ice. The male recipient dog is given pre-operative analgesia with oral carprofen and fentanyl patch 2 hours before surgery. Cephalic vein intravenous access is established. The animal is anesthetized (pre-anesthetics: atropine, 0.04 mg/kg, and telazol, 4 mg/kg; anesthetic: thiopental, 6-10 mg/kg), injected with heparin and placed in a warming blanket to preserve normothermia. Analgesia during surgery is provided by a bolus injection of 5 μg/kg fentanyl. Throughout surgery, anesthesia is maintained with isoflurane, 1-3% in 100% oxygen, delivered via an orotracheal tube. A neuromuscular blocking agent cisatracurium, 0.25 mg/kg, is given after depth anesthesia is established. The ECG is continuously recorded. An oral gastric tube is introduced for decompression and methylprednisolone, 500 mg, is given as initial imnmunosuppressive dose. Following thoracotomy and opening of the pericardium, the superior and inferior vena cava are looped with umbilical tapes and cannulated for venous drainage. The descending thoracic aorta is cannulated for arterial return and cardiopulmonary bypass initiated. The dog is maintained at 37-38° C. using a heater cooler within the cardiopulmonary bypass circuit. The aorta is cross-clamped and the heart removed, leaving a posterior remnant containing portions of the right and the left atria. The donor heart is sewn in using running, continuous 3-0 and 4-0 prolene suture. The atrial cuffs are joined first; the aorta and pulmonary artery anastomoses are then connected. The aortic clamp is removed and the heart is de-aired and allowed to recover. After reperfusion (⅓ of the time of cold ischemic period), the recipient is weaned off the extracorporeal circulation. Anticoagulation is reversed with protamine (1 mg/mg heparin given). Epicardial pacing wires and a chest tube are placed, thoracotomy closed in layers, air evacuated from the chest cavity and the tube secured to the skin. Vital signs (blood pressure, heart and respiratory rate, urine output and oxygen saturation) are monitored and recorded every hour for the first 4 hours and every two hours for the subsequent 14 hours. Arterial blood gases and electrolytes are periodically checked until the acidosis has resolved and the blood count has stabilized. Dogs remain on the ventilator overnight with Normosol-R intravenous drip, 2 ml/kg/h. On the morning of the first postoperative day, dogs that are hemodynamically stable are extubated.

B. Drug Administration

For analgesia, dogs receive a fentanyl transdermal patch, 75 μg/h, and carprofen, 4.4 mg/kg for 7 days postoperatively. Animals showing discomfort are further treated with buprenorphine, 0.02 mg/kg every 12 hours. The antibiotic cefazolin, 10 mg/kg is administered every 8 hours for 2 days. Beginning the day of transplantation, recipient dogs receive triple drug immunosuppression consisting of cyclosporine A, 18 mg/kg/day, azathioprine, 2 mg/kg/day, and methylprednisolone, 50 mg/day. The trough level of cyclosporine A is determined twice a week and immunosuppression is adjusted until a stable level of the agent is reached. Aspirin, 81 mg, is given daily to prevent venous thromboembolism.

C. Instrumentation

During transplantation, the recipient dog is chronically instrumented. A Tygon catheter is placed into the descending thoracic aorta to measure arterial pressure. Probes are implanted in the donor heart during extracorporeal circulation. A solid-state pressure gauge (Konigsberg) is inserted in the left ventricle through the apex. A Doppler-flow transducer is placed around the left circumflex coronary artery to measure blood flow and a pair of 3-MHz piezoelectric crystals are fixed on opposing endocardial surfaces at the base of the left ventricle. Wires and catheters are run subcutaneously to the intrascapular region. After recovery, dogs are trained to lie quietly on the laboratory table (64, 201-204).

D. Hemodynamics

Measurements are obtained at 10 days after each cell treatment and at sacrifice. The aortic catheter is connected to a P23 ID strain-gauge transducer to measure aortic pressure. LV pressure is determined and dP/dt is calculated. LV diameter is measured by connecting the implanted piezoelectric crystals to a transit time ultrasonic dimension gauge that generates a voltage linearly proportional to the transit time of the ultrasound traveling between the two crystals (1.55×μm/s). The analog signals are digitized at a sampling rate of 500 Hz. Systolic, diastolic, and mean arterial pressures, positive and negative dP/dt, heart rate, end-diastolic and end-systolic diameter, and pressure-diameter loop areas are evaluated (201-204).

E. Echocardiography

In conscious dogs, M-mode recordings are made from short axis views, with 21) guidance. LV chamber dimensions and wall thickness are measured in a plane below the mitral valve and perpendicular to the LV in an M-mode recording, LV chamber volume is assessed in a two-dimensional parasternal long axis view. LV volumes are calculated using the hemi-cylindrical hemi-ellipsoid model. Stroke volume is computed as the difference between LV end-systolic and end-diastolic volume. Cardiac output corresponds to the product of stroke volume and heart rate. Myocardial wall stress (WS) is calculated from the product of intraventricular pressure (LVP), radius of curvature (R) and wall thickness (h): WS=LVP×R/h.

F. Cell Infection

Progenitor cells (PCs) are infected with lentiviruses carrying EGFP (green), β-gal (blue) or RFP (red) so that the contribution of separate cell injections to the transplanted heart can be established quantitatively. In a separate set of studies, PCs to be injected are divided in three equal parts and infected respectively with lentiviruses carrying EGFP-Flag-tag under the cardiomyocyte specific α-MHC promoter, RFP-HA-tag under the SMC-specific Sm22a promoter and TFP-c-myc-tag under the EC-specific VE-cadherin promoter so that the generation of myocytes, smooth muscle cells (SMCs) and endothelial cells (ECs) in the transplanted heart are determined quantitatively by real-time RT-PCR and Western blotting by measuring the expression of the reporter constructs at the mRNA and protein level (57). These biochemical measurements are complemented with immunocytochemical determinations.

G. Cell Implantation

The intra-coronary route was selected to deliver the progenitor cells to the donor heart. This route was chosen to obviate the need for multiple survival surgeries that would be required with intramyocardial injection of cells. Experiments were performed in rats subjected to brief episodes of ischemia followed by reperfusion to document that progenitor cells cross the vessel wall and reach the myocardium (183). Ischemia typically occurs at transplantation (71). Movement of EGFP-tagged MPCs (green) was assessed ex vivo by two-photon microscopy after perfusion of the coronary vasculature with rhodamine labeled dextran (red). EGFP-labeled MPCs migrate across the wall of coronary vessels and within 3 hours move into the ischemic area (FIG. 9; see ref. 183 for detail). Thus, intra-arterial delivery of MPCs leads to their extravasation and homing to the myocardial interstitium.

In the transplanted dog, left Amplatz or right Judkins catheter is inserted into the left or right coronary artery under fluoroscopy. Cells are suspended in 0.5-2.0 mL of Isopaque and injected. The dye allows the visualization of the coronary vasculature and delivery of cells (FIG. 10). Then, the catheter is removed and the vessels repaired. Dogs are given antibiotics baytril, 6 mg/kg, and trimethoprim/sulfa, 33 mg/kg. Isopaque does not affect cardiac PC viability for as long as 16 hours. During the procedure, cardiac PCs are exposed to Isopaque for less than 5 min.

H. Generation of Immunocompatible Myocardium

In these initial studies, VPCs and MPCs were not separated and the PC pool was isolated from the explanted heart and expanded in vitro. Cells were infected with EGFP lentivirus (65% efficiency). Male EGFP-PCs were given 15 and 24 days after transplantation and the donor heart was examined 6 days after the second treatment, i.e., 30 days following surgery. The heart was sliced in 22 sections ˜4 mm each and several samples were obtained from each section (FIG. 11A): 114 samples were analyzed histologically. A similar protocol is used in all studies discussed in Examples 2-5. Clusters of newly formed EGFP-positive myocytes and coronary vessels (FIG. 11B-E) were detected in 109 of 114 specimens of the left and right ventricle. The ability of EGFP-PCs to differentiate into myocytes and SMCs was confirmed by detection of myocyte transcription factors, GATA4 and Nkx2.5, and the SMC transcription factor, GATA6 (FIG. 11F). The detection of the Y chromosome (Y-chr) confirmed the male genotype of the regenerated myocytes (FIG. 11G-H). As shown before, at most one X- and Y-chr were identified in the formed cells excluding cell fusion (FIG. 3). In contrast, at most 2 X-chr were seen in donor cardiac cells documenting their female genotype. The engraftment and survival of male EGFP-PCs was confirmed by PCR for EGFP DNA and the Sry gene located in the Y-chromosome (FIG. 11I and J). Random sampling of tissue from kidney, spleen, lung and liver failed to reveal DNA sequences for EGFP by PCR (FIG. 11I). Thus, at 15 and 6 days after the first and second injection no EGFP-PCs were found to be engrafted outside of the heart. Comparable findings were obtained in a second dog in which male EGFP-PCs were given 15 and 22 days after transplant and the animal was sacrificed 2 weeks later, i.e., 45 days after surgery.

I. Immunohistochemistry with Quantum Dots, FISH and Confocal Microscopy

The recognition of regenerated male myocardium within the female donor heart requires immunolabeling of structures and confocal microscopy. To evaluate the lineage commitment of differentiating cells, antibodies for the following proteins are utilized. Markers for myocytes include GATA4, Nkx2.5, MEF2C, α-SA, α-cardiac actinin, troponin I, troponin T, cardiac MHC, atrial and ventricular myosin light chain (MLC), connexin 43 and N-cadherin; for SMCs, GATA-6, TGF-β1 receptor, α-SMA and calponin; and for ECs, Ets1, Vezf, CD31 and vWf (14, 47, 48, 51, 57, 59, 64, 137, 139). Y- and X-chr are identified by FISH (14, 47, 51, 57, 139) with canine specific probes (Cambio).

Example 2 Implantation of BMPCs from the Recipient into the Transplanted Donor Heart Generates Immunocompatible Coronary Vessels and Mnyocytes Improving the Evolution of the Cardiac Graft

This Example demonstrates that bone marrow progenitor cells (BMPCs) can acquire the cardiomyocyte, and vascular smooth muscle cell (SMC) and endothelial cell (EC) lineages in support of the therapeutic efficacy of BMPCs. Additionally, the consequences of cell fusion events and paracrine effects on myocardial regeneration are addressed.

A. Transdifferentiation

To date, the hematopoietic stem cell appears to be the most versatile stem cell in crossing lineage boundaries and the most prone to break the law of tissue fidelity (40, 205). Early studies on BMPC differentiation into myocardium have generated great enthusiasm (47, 51, 52, 168) but other observations have rejected the initial results (41-43) and promoted a wave of skepticism about the therapeutic potential of BMPCs for the injured heart (46, 206). The major criticisms include inaccurate interpretation of the original data due to autofluorescence artifacts and the lack of genetic markers for the recognition of the donor BMPCs and their progeny (41-43, 46, 206).

To address these issues, female infarcted mice were injected with male BMPCs obtained from transgenic mice in which EGFP was under the control of the ubiquitous β-actin promoter and the consequences of this intervention on post-infarction remodeling were determined. In another set of experiments donor BMPCs were collected from male mice carrying EGFP or c-myc-tagged nuclear Akt transgene under the control of α-MHC promoter (FIG. 12A). Thus, the destiny of BMPCs within the recipient heart was determined by genetic tagging with EGFP, cell fate tracking with EGFP and c-myc, cell genotyping by sex-chr identification (FIGS. 12B and C), EGFP and c-mye gene detection by PCR, mRNA transcripts for EGFP and c-myc-tag by RT-PCR, and protein expression for EGFP and c-myc-tag by Western blotting. Additionally, a critical part of the experiments was the development of a methodology in which primary antibodies are directly labeled with quantum dots (36, 139, 207). This protocol eliminates the need for secondary antibody and avoids the interference of autofluorescence in the specificity of the reaction (57).

The results show that BMPCs integrate within the host heart where they establish temporary niches which create the microenvironment necessary for the engrafted cells to acquire the cardiac fate and form de novo myocardium (FIG. 13; 57). These data are consistent with our hypothesis and may offer mechanistic insights on the positive results recently obtained in double blind clinical trials (208, 209). These findings suggest that myocardial regeneration is a likely possibility and BMPCs may have implications for the treatment of the transplanted heart.

B. Cell Fusion

In several studies of myocardial regeneration, we have never found examples of fusion between BMPCs or other progenitor cells with resident cardiac cells (47, 48, 51, 59, 137, 139). We have investigated the possibility of cell fusion in several conditions by measuring the number of sex chromosomes in newly formed cardiomyocytes and coronary vessels (14, 47, 51, 57, 139, 217). For example, with this approach, we have excluded that male myocytes and vessels present in female transplanted hearts are the product of cell fusion (see FIG. 2). Additionally, we have employed the Cre-Lox genetic system to evaluate whether human MPCs can form human myocardium within the infarcted mouse or rat heart (139) and whether myocardial regeneration in these models is, at least in part, the product of fusion events. We have found no indication that cell fusion contributes to cardiac repair (FIG. 14). To exclude the possibility that heterokaryons are formed when the donor hear is colonized with recipient progenitor cells, the number of sex chromosomes is measured in the newly formed structures to assess the participation of cell fusion in myocardial regeneration.

C. Paracrine Effects

We test the possibility of a paracrine effect of administered progenitor cells by giving BrdU chronically after transplantation by a well established protocol (51, 57, 139). Over time, cumulative BrdU labeling of female myocytes and coronary vessels provides a quantitative measurement of the cellular responses of the donor heart to the injection of recipient male progenitor cells. Additionally, the fraction of cycling female myocytes, ECs and SMCs at sacrifice is determined by Ki67, MCNM5 and phospho-H3 labeling to assess the characteristics of the donor myocardium at the end of the study. Finally, the number of female myocytes and vessels is determined to define the composition of the donor heart and its changes with time. The injected cells could also attenuate cell death mechanisms. Thus, apoptosis of EGFP-, β-Gal- or RFP-negative and Y-chr negative cells is measured. Similarly, the contribution of male myocytes and vessels to the restoration of immunocompatible structures within the non-immunocompatible myocardium is evaluated.

D. Implantation of BMPCs in Transplanted Donor Heart in Canines

(1) Cell Preparation

The bone marrow is harvested from the iliac crests through a Jamshidi needle (13G×2″) (218); ˜10 ml of bone marrow is obtained. This protocol yields a total of 20×10⁸ mononuclear cells in each recipient dog. Following lysis of red blood cells in NH4Cl/K, cells are enriched by equilibrium centrifugation over a cushion of Ficoll-Hypaque-400 at a density of 1.077 g/ml. For lineage-depletion, mononuclear cells are incubated with immunomagnetic beads conjugated with monoclonal antibodies for CD3 (T lymphocytes), CD20 (B lymphocytes), CD33 (myeloid progenitors), CD14 and CD15 (monocytes). The lineage-negative fraction is exposed to c-kit-conjugated-immunobeads (clone AC126). A small aliquot is analyzed by FACS to confirm the purity of the preparation (47, 168). Cells are stained with c-kit-A3C6E2 antibody that does not cross-react with the epitope recognized by the AC126 antibody; ˜10×10⁶ c-kit-positive BMPCs are collected from each recipient dog. Since at most 5 injections of BMPCs is done in each dog, 2×10⁶ cells are injected each time.

(2) Intervals

One month after transplantation, dogs are anesthetized for left heart catheterization and cell injection (Group 1; EGFP-labeled cells). This protocol is then applied twice for the next month (Group 2; β-Gal-labeled cells) and subsequently twice for an additional month (Group 3; RFP-labeled cells). Group 1 animals are sacrificed one month after a single cell injection, 2 months after transplantation; Group 2 animals are sacrificed one month after the last of 3 cell injections, 3 months after transplantation; and Group 3 animals are sacrificed one month after the last of 5 cell injections, 4 months after transplantation. Another group of animals, Group 4, is injected bi-weekly for 2 months (5 injections) with BMPCs infected with three lentiviruses carrying reporter genes driven by cell lineage specific promoters. These animals are sacrificed 4 months after transplantation mimicking Group 3. The end-points indicated here are formulated to evaluate the progressive accumulation of immunocomnpatible myocardium. In Groups 1-3, BrdU is injected twice a day (50 mg/kg b.w.×2) to label forming cells over time (64).

(3) Immunocompatible Myocytes and Coronary Vessels

Three methods are used to detect immunocompatible myocytes and vessels within the donor heart: a) Genetic tagging/clonal marking; b) Real-time RT-PCR and Western blotting for reporter genes; and c) Structural analysis. Because of these objectives, at sacrifice the donor heart is subdivided into two parts: one for genetic tagging and biochemical analysis of BMPC transdifferentiation and the second for the quantitative characterization of the contribution of donor and regenerated recipient myocardium to the transplanted heart.

a) Genetic tagging/clonal marking (see Example 4): The objective is to document whether the site of integration of the EGFP, β-gal and RFP lentivirus in BMPCs is found in the committed progeny. This demonstrates that BMPCs transdifferentiate and have the ability to form de novo myocardium.

b) Real-time RT-PCR and Western blotting for reporter genes (see Example 4).

c) Structural analysis (see Example 3): The morphomnetric approach developed in our laboratory allows us to measure the proportion of newly formed male myocardial structures and resident female myocardium.

The results of these experiments in canines is expected to show that BMPCs isolated from the recipient male dog will differentiate into myocytes, smooth muscle cells, and endothelial cells and generate immunocompatible myocardium and myocardial vessels in the female donor heart. No evidence of fusion events between the male bone marrow progenitor cells and the donor female myocardial cells is expected to be observed.

Example 3 Implantation of Vascular Progenitor Cells from the Recipient into the Transplanted Donor Heart Generates Immunocompatible Coronary Vessels Improving the Evolution of the Cardiac Graft

Cardiac allograft vasculopathy (CAV) is a major pathological event which severely affects the unfavorable evolution of the transplanted heart (72, 85, 91-93, 108, 109). In this Example, the therapeutic potential of vascular progenitor cells (VPCs) is defined. This cell category is the most powerful for the replacement of the coronary circulation of the donor heart with immunocompatible vessels and thus, the possibility to introduce stem cell therapy for the treatment of coronary artery disease is dramatically advanced. Moreover, the documentation that progenitor cells with angiogenic properties reside in the heart questions the notion that the bone marrow is the exclusive reservoir or source of stem cells for therapeutic vasculogenesis and points to VPCs as the cell of choice for biological bypass. Two issues are addressed in this Example: cell engraftment and necessity to create the various portions of the coronary circulation.

A. Engraftment

The criteria that govern myocardial regeneration and replacement of damaged non-immunocompatible tissue with functionally competent immunocompatible myocardium involve the ability of the delivered progenitor cells to home to or in proximity of the injured sites together with the permissive behavior of the donor myocardium (47, 48, 50-53, 59, 137, 139, 173, 221). These variables dictate the number of cells that actually engraft within the hostile environment of the target organ which, in turn, condition the efficacy of cell therapy. Engraitment necessitates a surrounding where the cells can survive, divide and differentiate (64, 163, 165-167). Based on data with BMPCs (57) and treated transplanted hearts (FIG. 15), cell engraftment is completed in a few days. Junctional and adhesion proteins are present on the implanted cells documenting a successful interaction between progenitor cells and resident cells; connexin 43 and 45, and N- and E-cadherin have been found between progenitor cells and myocytes or fibroblasts which operate as supporting cells (57, 137, 169). Also, apoptosis occurs in non-engrafted cells and cell division occurs in engrafted cells (FIG. 17). Thus, the destiny of VPCs is established by measuring cell death and proliferation and their integration with resident cardiac cells 2-5 days after injection.

B. Coronary Vasculature

The identification and characterization of a coronary VPC discussed above raises the possibility that the heart harbors a coronary VPC which regulates the turnover, growth and differentiation of the coronary circulation. To test this possibility, human VPCs were infected with a lentivirus expressing EGFP and were subsequently examined for the ability to create functionally competent coronary vessels in dogs with critical coronary artery stenosis. These VPCs formed human conductive and intermediate-sized coronary arteries together with small resistance arterioles and capillary profiles within the immunosuppressed recipient myocardium, restoring in part myocardial blood flow to the distal portion of the heart (FIG. 16). Thus, VPCs may be implemented for the replacement of coronary vessels affected by allograft vasculopathy in the transplanted dog heart.

As described in Example 2 with BMPCs, at most 5 injections of VPCs are done in each dog; 2×10⁶ cells are injected each time.

C. Analysis of the Transplanted Heart

At sacrifice the donor heart is subdivided into two parts: one for the identification by genetic tagging/clonal marking and biochemical-molecular parameters of progenitor cell differentiation in cardiac lineages (see Example 4) and the second for the quantitative characterization of the contribution of donor and regenerated recipient myocardium to the transplanted heart discussed below.

The first portion of the heart is enzymatically digested (see Example 4). The second portion of the heart is utilized for the evaluation of myocytes and coronary vessels of donor and recipient origin. A branch of the coronary artery is cannulated and the heart and coronary vasculature is fixed by perfusion with formalin. Briefly, the chest is opened, 20,000 units of heparin is given intravenously, and vessels originating from the aortic arch is ligated. The heart is arrested in diastole, the descending aorta ligated and cannulated. The heart is perfused with phosphate buffer and before perfusion with formalin, a portion of the heart is removed for cell isolation and the studies discussed in Example 4 (64, 232-237). The expression of EGFP, β-gal or RFP together with the localization of the Y-chromosome allows us to distinguish structures mediated by growth and differentiation of progenitor cells at different time points following cardiac transplantation. In contrast, cardiomyocytes and coronary vessels negative for these reporter proteins and showing the female genotype constitute the remaining component of the donor myocardium.

D. Cell Engraftment

The ability of male EGFP-, β-gal- and RFP-tagged VPCs to home and form junctional complexes with resident female cardiac cells is determined as previously performed (57, 137, 139, 169). This analysis includes the identification of connexin 43, connexin 45, N-cadherin, E-cadherin, and L-selectin. The number of actually engrafted cells is measured quantitatively (57).

E. Cell Growth and Death

The progeny of the injected cells is recognized by the presence of EGFP, β-gal and RFP. This labeling is combined with the detection of BrdU indicative of newly formed cells and cumulative growth (169). This measurement is complemented by the expression of MCM5, Ki67 and phospho-H3 to recognize the fraction of cycling cells (MCM5, Ki67) and in mitosis (phospho-H3). The degree of apoptosis and necrosis in VPCs and their progeny is also measured (139, 169, 232-237).

F. Coronary Vasculature and Cardiomyocytes

Morphometric measurements of coronary vessels require a specific approach. This technique and its theoretical principles have been previously described (136). This protocol applies to the analysis of capillaries as well (40, 47, 48, 59). Classes of vessels positive for EGFP, β-gal or RFP together with the Y-chromosome is measured separately. An identical analysis is conducted in vessels which are negative for these markers. Thus, an estimation of the immunocompatible and non-immunocompatible coronary vasculature is obtained.

The number of newly formed and existing myocytes is measured quantitatively by a protocol developed previously which includes measurements in tissue sections and isolated cells (136). Sampling for coronary circulation and cardiomyocytes: see ref. 136.

The results of these experiments are expected to show that vascular progenitor cells isolated from the explanted heart of the male recipient dog will engraft in the donor female heart after administration and differentiate into predominantly smooth muscle cells and endothelial cells. The differentiated cells will assemble into immunocompatible coronary vasculature (coronary arteries, arterioles, and capillaries) similar to that formed after the administration of human vascular progenitor cells (see section B above).

Example 4 Implantation of MPCs from the Recipient into the Transplanted Donor Heart Generates Immunocompatible Cardiomyocytes Improving the Evolution of the Cardiac Graft

Myocyte progenitor cells (MPCs) are programmed to give rise to cardiomyocytes and these cells should be superior to bone marrow progenitor cells (BMPCs) and vascular progenitor cells (VPCs) for replacement of lost muscle mass. This is suggested by in vitro results in which the differentiated progenies of MPCs and VPCs were compared (see FIG. 7). BMPCs differentiate into myocytes (239-241), smooth muscle cells (242, 243) and endothelial cells (244, 245) in vitro. However, the relative proportion of these cell types in the same preparation is difficult to obtain.

To address the issue of the regenerative capacity of the different progenitor cell classes (e.g. BMPCs, MPCs, and VPCs), the quantitative measurements of newly formed myocytes and vessels based on morphometric principles and immunolabeling (Example 3) is complemented with a novel genetic-molecular assay developed previously in our laboratory (246). Thus, two complementary methods are used: a genetic-molecular assay and a structural assay. Genetic tagging is discussed below together with a series of other molecular determinations.

A lentivirus expressing EGFP, β-gal and RFP is employed for in vitro infection of BMPCs, VPCs and MPCs. The detection of the lentiviral integration site is based on the premise that it contains two restriction enzyme (RE) cleavage sites at a reasonable distance (50-2000 bp) from the lentiviral LTRs located at the 3′ and 5′ sites of the viral genome. Following the cleavage of the genomic DNA with the RE, DNA products are self-ligated to produce circularized DNA. This step creates a genomic sequence of a length that is variable in view of the random location of the RE site within the region of the dog genome flanking the viral DNA. The unknown lentiviral flanking region is entrapped between two known sequences and can be, therefore, amplified by PCR and resolved on gel; each band corresponds to one insertion site. Data have been obtained after intramyocardial injection of human cardiac progenitor cells in immunosuppressed infarcted rats to validate this novel approach (246; FIG. 17).

The data indicate that similarities exist between forming myocardium (36, 51, 57, 59, 64, 139) and late-fetal and postnatal cardiac maturation (136, 247, 248). The volume of myocytes is comparable although differences in number exist; regeneration tends to recapitulate the processes present in the fetal-neonatal heart (249, 250). Accordingly, the prenatal and postnatal heart are used for comparison.

Hearts from female donors are transplanted into male recipients as described in Example 1. Progenitor cells isolated from the male explanted heart are infected with lentivirus carrying EGFP, β-gal and RFP. The infected progenitor cells are then injected into the transplanted donor heart. At most 5 injections of progenitor cells are done in each dog; 2×10⁶ cells are injected each time.

Molecular assays and immunocytochemistry are used to identify the time-course of myocardial regeneration in the transplanted heart and in the developing heart (fetal dog heart at 40 and 60 days of gestation, 1-2 days after birth, at the time of weaning, 4-5 weeks, and 8 months). The expression of transcription factors that control myogenesis and vasculogenesis is determined (247, 248, 251-253). Moreover, membrane and cytoplasmic proteins specific of myocytes, smooth muscle cells and endothelial cells are studied (254-257). Molecular and cytochemical detections are both relevant to obtain information with two complementary methods and ensure that protein expression is properly distributed within cells. Postnatally, apoptosis decreases rapidly and this adaptation is paralleled by a reduction in myocyte formation coupled with binucleation of the enlarging myocytes (258-260). Myocyte karyokinesis in the absence of cytokinesis is accompanied by downregulation of the transcription factor Tsc (tuberous sclerosis complex) and upregulation of Gax (growth arrest gene). Similar adaptations may occur in the transplanted heart.

Transplanted Heart: At sacrifice, in a portion of the heart, a coronary artery branch is cannulated and cardiac cells are enzymatically dissociated with collagenase for biochemical-molecular determinations (232-237). Large myocytes of donor origin and small cardiac cells (newly formed myocytes and non-myocytes) of both donor and recipient origin are separated by Ficoll gradient and differential centrifugation (246). Within the small cells, the progeny of the injected progenitor cells are sorted by FACS based on the presence of EGFP, β-gal and RFP. The spontaneous fluorescence of EGFP- and RFP-positive cells allow their direct collection. When β-gal-positive progenitor cells are injected, the isolated cells are fixed in 4% paraformaldehyde for 15 min, stained with anti β-gal antibody (168) and sorted by FACS. Cells are employed directly for RNA extraction and real-time RT-PCR. For genetic tagging, an additional step is required. Progenitor cells are sorted by FACS on the basis of c-kit and flk1 expression (47, 59, 64, 139). C-kit-negative cells are subdivided in CD31-positive (endothelial cells), calponin-positive (smooth muscle cells), ac-SA-positive (myocytes) and procollagen-I-positive (fibroblasts) cells.

Genetic tagging: Genomic DNA is extracted and employed for the detection of the site of viral integration. Importantly, each cell population isolated from each heart is processed separately according to the AKANE protocol (see FIG. 17 and legend). Primers are designed to include a portion of the coding regions of EGFP, β-gal and RFP to distinguish the three viral genomes. Amplified DNA is run on agarose gel. Bands are cut, DNA extracted and sequenced from both ends to determine the insertion site of each clone (246).

Biochemical-molecular determinations: These analyses are performed in freshly isolated EGFP-, β-gal- and RFP-positive cells and whole lysates of fetal, neonatal and young adult hearts by real time RT-PCR (139, 263). Western blotting is also employed. These analyses are complemented by the detection of proteins by immnunocytochemistry. For real-time RT-PCR, total RNA is extracted with Trizol or RecoverAll™ Total Nucleic Acid Isolation Ambion Kit which is designed for formalin/paraformaldehyde fixed structures (139, 263).

Changes in expression of transcription factors involved in differentiation of myocytes (Nkx2.5, GATA4, MEF2C, Tbx, SRF, HAND-1, HAND-2), smooth muscle cells (GATA6) and endothelial cells (Ets1, Vezf1) are determined. Moreover, mRNA expression of membrane and cytoplasmic components specific of myocytes (connexin 43, N-cadherin, troponin I, atrial and ventricular MLC-2, α- and β-MHC, α-SA), smooth muscle cells (α-SMA, TGF-βR) and endothelial cells (eNOS, CD31, vWf) is studied. For mnyocyte karyokinesis and cytokinesis, Tsc and Gax expression is determined.

PCR for Y-chromosome DNA: Primers are employed to detect Sry, the sex determining region of the Y-chromosome: dogSry-F: 5′-CGTTGGAACGGACAATTCAACCTCGAA-3 SEQ ID NO.: 1 (26 nt, Tm 61° C.) and dogSry-R: 5′-ACCTGCTTCATAGCATGGAGGAGGA-3′ SEQ ID NO.: 2 (26 nt, Tm 64° C.) [amplicon size: 369 bp].

Ilmmunocytochemistry: These analyses are conducted by confocal microscopy of isolated cells and developing heart to complement the real-time RT-PCR studies.

The results of this set of experiments is expected to show the myocyte progenitor cells will generate predominantly new myocytes of recipient origin, while vascular progenitor cells will generate predominantly smooth muscle cells and endothelial cells of recipient origin. The bone marrow progenitor cells will generate myocytes, smooth muscle cells, and endothelial cells of recipient origin, but are expected to generate fewer numbers of myocytes than myocyte progenitor cells. It is also expected that the generation of immunocompatible myocardium by the implanted progenitor cells will be comparable to the formation of myocardial tissue during development.

Example 5 Implantation of VIPCs and MPCs into the Transplanted Donor Heart Generates Immunocompatible Coronary Vessels and Cardiomyocytes which Together Reconstitute an Immunocompatible Heart

The objective of this Example is to utilize therapeutically the two recently identified progenitor cell classes, vascular progenitor cells (VPCs) and myocyte progenitor cells (MPCs), to replace donor myocardium with new recipient myocardium. This approach takes advantage of the vessel regenerative capacity of VPCs and myocyte formation of MPCs to dramatically restructure the transplanted heart. Human studies on cardiac chimerism (14-26) are consistent with this possibility and, in fact, point strongly in this direction. The premise is that resident MPCs and VPCs are preferable and more efficient in creating de novo myocardium than bone marrow progenitor cells (BMPCs) which have to transdifferentiate and acquire a different genetic phenotype (36, 185, 186, 207) before committing to the myocyte and vascular cell lineages (47-57). However, progenitor cells from the explanted organ and/or the bone marrow can be employed to rebuild the donor heart.

Three protocols are used to assess whether the implanted progenitor cells generate functional myocardial tissue and vessels: regional ventricular function, coronary blood flow, and myocyte mechanics.

A. Ventricular Function

The use of a large animal model offers the unique opportunity to instrument the transplanted heart with sonomicrometers and determine chronically the time course of the alterations in regional function and establish whether delivery of progenitor classes results in an improvement of the dyskinetic and hypokinetic segments included within the sonomicrometers (64, 232-237). Recovery of contraction points to myocardial regeneration as one of the possible mechanisms involved, while the lack of amelioration in function suggests absence of tissue reconstitution. The histological examination of the same regions at sacrifice allows us to obtain critical information on the structure and function of the transplanted heart.

B. Coronary Blood Flow (CBF) and Hemodynamics

The potential efficacy of cell therapy requires the inclusion of measurements of CBF distribution and coronary vascular resistance (264-267). If the formation of the various segments of the coronary circulation by BMPCs, VPCs and/or MPCs occurs and cardiac allograft vasculopathy (CAV) is partly corrected, a functional counterpart has to be documented. The collateral circulation of the canine heart protects to a certain extent the myocardium from ischemic events (264-267) so that coronary occlusion may result in hypokinesis instead of dyskinesis of the affected region of the heart (64). Therefore, the potentiation of collateral vessel formation has to be considered and carefully analyzed together with angiogenesis and vasculogenesis to interpret properly functional changes in CBF (FIG. 18). Data are obtained at days after each cell treatment and at sacrifice (264, 265, 268-270).

C. Myocyte Mechanics

An important aspect of the reconstituting myocardium concerns the performance of regenerated myocytes. Thus, parameters of myocyte contractility, calcium handling and L-type calcium current are measured in isolated myocytes and comparisons are made with donor myocytes (40, 57, 59, 139, 271). The acquisition of this information allows us to establish the effective functional competence of regenerated cells (59, 139). Changes in myocyte mechanics which accompany the acquisition of the adult phenotype are assessed and analyzed in myocyte populations derived from different progenitor classes. Thus, the most efficient and powerful myocyte progeny are identified. These measurements are routinely performed (40, 57, 59, 139, 271).

D. Specific Methods

Intervals: As discussed in Example 2, during the course of the study, dogs are anesthetized for left heart catheterization and autologous progenitor cell injection (Group 1; 50% EGFP-labeled VPCs and 50% RFP-labeled MPCs). This protocol is then applied bi-weekly for the next month (Group 2; 50% EGFP-labeled VPCs and 50% β-Gal-labeled MPCs) and subsequently for an additional month (Group 3; 50% EGFP-labeled VPCs and 50% β-Gal-labeled MPCs). Group 1 animals are sacrificed one month after a single cell injection, 2 months after transplantation; Group 2 animals are sacrificed one month after the last of 3 cell injections, 3 months after transplantation; and Group 3 animals are sacrificed one month after the last of 5 cell injections, 4 months after transplantation. Another group of animals, Group 4, is injected bi-weekly for 2 months (5 injections) with 50% MPCs infected with a lentivirus carrying EGFP-Flag-tag under the cardiornyocyte specific α-MHC promoter, RFP-HA-tag under the SMC-specific Sm22a promoter and TFP-c-myc-tag under the EC-specific VE-cadherin promoter. These animals are sacrificed 4 months after transplantation. At most 5 injections of progenitor cells are done in each dog; 2×10⁶ cells are injected each time.

CBF: Two ml of Steri spheres (BioPal) suspension (2 millions/mL) are mixed with arterial blood and injected into left atrium over 5 seconds. Immediately before the injection, arterial blood reference sample is withdrawn from the aortic catheter. At the end of experiment, transmural tissue samples (˜1 g) are harvested from cardiac regions of interest and cut into three layers: epicardial, mid-myocardial and endocardial. Tissue and reference blood samples are dried overnight, and then shipped to Bio-Pal for neutron activation and radioactivity counting. The average radioactivity counts for myocardium are calculated as Ci=(C1×W1+C2×W2+C3×W3)/(W1+W2+W3) where Ci is the average count (dpm/g), C1-3 and W1-3 are the counts and wet weights for the epicardium, mid-myocardium, and endocardium layers, respectively. The myocardial flow is calculated as Qi=(Ci/Cref)×R(ml/min) where Qi is flow, Ci and Cref are the radioactivities in tissue and in blood reference sample, respectively, and R is the withdrawal rate of the reference blood sample. Endocardial/epicardial flow ratio is calculated to obtain an index of regional flow pattern (268-270).

Mechanics, Ca2+ transients and electrophysiology (see FIG. 19): Myocytes are transferred to a chamber placed on the stage of an inverted microscope. External bath Ca2+ is kept at 1.5 mM. Mechanics, Ca2+ transients: Myocytes are stimulated at 1.0 Hz by rectangular depolarizing pulses, 2 ms in duration, and twice-diastolic threshold intensity. Changes in cell length are quantified by edge tracking. Sarcomere length is determined by the mean frequency of sarcomere spacing utilizing the Fast Fourier Transform. Fluo 3-fluorescence is measured by epi-illumination with flashes of 488 nm light. After loading cell with the Ca2+ probe, experiments are performed at 25±0.2° C. to minimize the loss of the Ca2+ indicator. The ability of myocytes to adapt to different rates of stimulation and extracellular Ca2+ concentrations is examined (40, 59). Electrophysiology: Electrical properties of differentiating myocytes are measured in combination with cell shortening. Data are collected by whole cell patch-clamp technique in voltage- and current-clamp mode and by edge motion detection measurements. Voltage, time-dependence and density of L-type Ca2+ current is analyzed in voltage-clamp preparations. T-type Ca2+ current is assessed (265); it is restricted to developing myocytes (272). Relationship between shortening and action potential is done in current-clamp mode (57, 271, 273-280).

The results of these experiments are expected to show that the implanted MPCs will generate predominantly immunocompatible myocytes, while the imnplanted VPCs will generate predominantly immnnocompatible smooth muscle cells and endothelial cells. Some of the smooth muscle cells and endothelial cells derived from the recipient will assemble into functional coronary vessels that may reduce cardiac allograft vasculopathy and enhance coronary blood flow.

Having thus described in detail preferred embodiments of the present invention, it is to be understood that the invention defined by the appended claims is not to be limited by particular details set forth in the above description as many apparent variations thereof are possible without departing from the spirit or scope thereof.

Those skilled in the art will recognize, or be able to ascertain using no more than routine experimentation, many equivalents to the specific embodiments of the invention described herein. Such equivalents are intended to be encompassed by the following claims.

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The invention claimed is:
 1. A method of reducing an immune response to a transplanted donor heart in a recipient subject comprising: administering isolated adult bone marrow progenitor cells to the transplanted donor heart, wherein said adult bone marrow progenitor cells are isolated from the recipient subject's bone marrow and are lineage negative and c-kit positive, and administering isolated vascular progenitor cells to the transplanted donor heart, wherein said vascular progenitor cells are isolated from the recipient subject's myocardial tissue and are lineage negative, c-kit positive, and vascular endothelial growth factor receptor 2 (VEGFR2) positive, wherein said bone marrow progenitor cells generate immunocompatible myocardium and immunocompatible myocardial vessels and said vascular progenitor cells generate immunocompatible vessels following their administration, thereby reducing the immune response to said transplanted donor heart.
 2. The method of claim 1, wherein said bone marrow progenitor cells differentiate into immunocompatible endothelial cells, smooth muscle cells, and cardiomyocytes.
 3. The method of claim 1, wherein said bone marrow progenitor cells are activated by exposing the cells to one or more cytokines prior to administration.
 4. The method of claim 1, wherein said bone marrow progenitor cells are administered immediately after transplantation.
 5. The method of claim 1, further comprising administering to the subject an immunosuppressive therapy.
 6. The method of claim 1, wherein said subject is human.
 7. The method of claim 1, wherein said adult bone marrow progenitor cells are expanded in culture prior to administration to the donor heart.
 8. The method of claim 1, wherein said vascular progenitor cells are administered to the transplanted donor heart following the administration of said bone marrow progenitor cells.
 9. The method of claim 1, further comprising administering isolated myocyte progenitor cells to the transplanted donor heart, wherein said myocyte progenitor cells are isolated from the recipient subject's myocardial tissue and are lineage negative, c-kit positive, and VEGFR2 negative, and wherein said myocyte progenitor cells differentiate into immunocompatible cardiomyocytes.
 10. The method of claim 9, wherein said vascular progenitor cells and/or said myocyte progenitor cells are administered to the transplanted donor heart by multiple administrations after transplantation.
 11. The method of claim 10, wherein said multiple administrations occur at a set interval after administration of said bone marrow progenitor cells.
 12. The method of claim 9, wherein said adult bone marrow progenitor cells, said vascular progenitor cells, and/or said myocyte progenitor cells are administered to the transplanted donor heart by intramyocardial or intracoronary injection. 